Regulating metabolism by modifying the level of trehalose-6-phosphate

ABSTRACT

Method for the inhibition of carbon flow in the glycolytic direction in a cell by increasing the intracellular availability of trehalose-6-phosphate.

CROSS-REFERENCE TO RELATED APPLICATIONS

This application is a continuation of U.S. patent application Ser. No. 11/818,157 filed on Jun. 13, 2007, which is a divisional of U.S. patent application Ser. No. 10/682,456 filed on Oct. 9, 2003, which is a division of U.S. patent application Ser. No. 09/171,937 filed on Apr. 28, 1999, which is a national state application of International Application PCT/EP97/02497 filed on May 2, 1997, and claims priority to Netherlands Application No. EP96201225.8 filed May 3, 1996, Netherlands Application No. EP96202128.3 filed Jul. 26, 1996, and Netherlands Application No. EP96202395.8 filed Aug. 29, 1996, each of which is incorporated by reference by its entirety.

FIELD OF THE INVENTION

Glycolysis has been one of the first metabolic processes described in biochemical detail in the literature. Although the general flow of carbohydrates in organisms is known and although all enzymes of the glycolytic pathway(s) are elucidated, the signal which determines the induction of metabolism by stimulating glycolysis has not been unravelled. Several hypotheses, especially based on the situation in yeast have been put forward, but none has been proven beyond doubt.

Influence on the direction of the carbohydrate partitioning does not only influence directly the cellular processes of glycolysis and carbohydrate storage, but it can also be used to influence secondary or derived processes such as cell division, biomass generation and accumulation of storage compounds, thereby determining growth and productivity.

Especially in plants, often the properties of a tissue are directly influenced by the presence of carbohydrates, and the steering of carbohydrate partitioning can give substantial differences.

The growth, development and yield of plants depends on the energy which such plants can derive from CO₂-fixation during photosynthesis.

Photosynthesis primarily takes place in leaves and to a lesser extent in the stem, while other plant organs such as roots, seeds or tubers do not essentially contribute to the photoassimilation process. These tissues are completely dependent on photosynthetically active organs for their growth and nutrition. This then means that there is a flux of products derived from photosynthesis (collectively called “photosynthate”) to photosynthetically inactive parts of the plants.

The photosynthetically active parts are denominated as “sources” and they are defined as net exporters of photosynthate. The photosynthetically inactive parts are denominated as “sinks” and they are defined as net importers of photosynthate.

It is assumed that both the efficiency of photosynthesis, as well as the carbohydrate partitioning in a plant are essential. Newly developing tissues like young leaves or other parts like root and seed are completely dependent on photosynthesis in the sources. The possibility of influencing the carbohydrate partitioning would have great impact on the phenotype of a plant, e.g. its height, the internodium distance, the size and form of a leaf and the size and structure of the root system.

Furthermore, the distribution of the photoassimilation products is of great importance for the yield of plant biomass and products. An example is the development in wheat over the last century. Its photosynthetic capacity has not changed considerably but the yield of wheat grain has increased substantially, i.e. the harvest index (ratio harvestable biomass/total biomass) has increased. The underlying reason is that the sink-to-source ratio was changed by conventional breeding, such that the harvestable sinks, i.e. seeds, portion increased. However, the mechanism which regulates the distribution of assimilation products and consequently the formation of sinks and sources is yet unknown. The mechanism is believed to be located somewhere in the carbohydrate metabolic pathways and their regulation. In the recent research it has become apparent that hexokinases may play a major role in metabolite signalling and control of metabolic flow. A number of mechanisms for the regulation of the hexokinase activity have been postulated (Graham et al. (1994), The Plant Cell 6: 761; Jang & Sheen (1994), The Plant Cell 6, 1665; Rose et al. Eur. J. Biochem. 199, 511-518, 1991; Blazquez et al. (1993), FEBS 329, 51; Koch, Annu. Rev. Plant Physiol. Plant. Mol. Biol. (1996) 47, 509; Jang et al. (1997), The Plant Cell 9, 5, one of these theories of hexokinase regulation, postulated in yeast mentions trehalose and its related monosaccharides (Thevelein & Hohmann (1995). TIBS 20, 3). However, it is hard to see that this would be an universal mechanism, as trehalose synthesis is believed to be restricted to certain species.

Thus, there still remains a need for the elucidation of the signal which can direct the modification of the development and/or composition of cells, tissue and organs in vivo.

SUMMARY OF THE INVENTION

It has now been found that modification of the development and/or composition of cells, tissue and organs in vivo is possible by introducing the enzyme trehalose-6-phosphate synthase (TPS) and/or trehalose-6-phosphatase phosphate (TPP) thereby inducing a change in metabolic pathways of the saccharide trehalose-6-phosphate (T-6-P) resulting in an alteration of the intracellular availability of T-6-P. Introduction of TPS thereby inducing an increase in the intracellular concentration of T-6-P causes inhibition of carbon flow in the glycolytic direction, stimulation of the photosynthesis, inhibition of growth stimulation of sink-related activity and an increase in storage of resources. Introduction of TPP thereby introducing a decrease in the intracellular concentration of T-6-P causes stimulation of carbon flow in the glycolytic direction, increase in biomass and a decrease in photosynthetic activity.

The levels of T-6-P may be influenced by genetic engineering of an organism with gene constructs able to influence the level of T-6-P or by exogenously (orally, topically, parenterally etc.) supplying compounds able to influence these levels.

The gene constructs that can be used in this invention are constructs harboring the gene for trehalose phosphate synthase (TPS) the enzyme that is able to catalyze the reaction from glucose-6-phosphate and UDP-glucose to T-6-P. On the other side a construct coding for the enzyme trehalose-phosphate phosphatase (TPP) which catalyzes the reaction from T-6-P to trehalose will, upon expression, give a decrease of the amount of T-6-P.

Alternatively, gene constructs harboring antisense TPS or TPP can be used to regulate the intracellular availability of T-6-P.

Furthermore, it was recently reported that an intracellular phospho-alpha-(1,1)-glucosidase, TreA, from Bacillus subtilis was able to hydrolyse T-6-P into glucose and glucose-6-phosphate (Sch{hacek over (o)}ck et al., Gene, 170, 77-80, 1996). A similar enzyme has already been described for E. coli (Rimmele and Boos (1996), J. Bact. 176 (18), 5654-).

For overexpression heterologous or homologous gene constructs have to be used. It is believed that the endogenous T-6-P forming and/or degrading enzymes are under allosteric regulation and regulation through covalent modification. This regulation may be circumvented by using heterologous genes.

Alternatively, mutation of heterologous or homologous genes may be used to abolish regulation.

The invention also gives the ability to modify source-sink relations and resource allocation in plants. The whole carbon economy of the plant, including assimilate production in source tissues and utilization in source tissues can be modified, which may lead to increased biomass yield of harvested products. Using this approach, increased yield potential can be realized, as well as improved harvest index and product quality. These changes in source tissues can lead to changes in sink tissues by for instance increased export of photosynthase. Conversely changes in sink tissue can lead to change in source tissue.

Specific expression in a cell organelle, a tissue or other part of an organism enables the general effects that have been mentioned above to be directed to specific local applications. This specific expression can be established by placing the genes coding for TPS, TPP or the antisense genes for TPS or TPP under control of a specific promoter.

Specific expression also enables the simultaneous expression of both TPS and TPP enzymes in different tissues thereby increasing the level of T-6-P and decreasing the level of T-6-P locally.

By using specific promoters it is also possible to construct a temporal difference. For this purpose promoters can be used that are specifically active during a certain period of the organogenesis of the plant parts. In this way it is possible to first influence the amount of organs which will be developed and then enable these organs to be filled with storage material like starch, oil or proteins.

Alternatively, inducible promoters may be used to selectively switch on or off the expression of the genes of the invention. Induction can be achieved by for instance pathogens, stress, chemicals or light/dark stimuli.

DEFINITIONS

Hexokinase activity is the enzymatic activity found in cells which catalyzes the reaction of hexose to hexose-6-phosphate. Hexoses include glucose, fructose, galactose or any other C₆ sugar. It is acknowledged that there are many isoenzymes which all can play a part in said biochemical reaction. By catalyzing this reaction hexokinase forms a key enzyme in hexose (glucose) signalling.

Hexose signalling is the regulatory mechanism by which a cell senses the availability of hexose (glucose).

Glycolysis is the sequence of reactions that converts glucose into pyruvate with the concomitant production of ATP.

Cold sweetening is the accumulation of soluble sugars in potato tubers after harvest when stored at low temperatures.

Storage of resource material is the process in which the primary product glucose is metabolized into the molecular form which is fit for storage in the cell or in a specialized tissue. These forms can be divers. In the plant kingdom storage mostly takes place in the form of carbohydrates and polycarbohydrates such as starch, fructan and cellulose, or as the more simple mono- and di-saccharides like fructose, sucrose and maltose; in the form of oils such as arachic or oleic oil and in the form of proteins such as cruciferin, napin and seed storage proteins in rapeseed. In animal cells also polymeric carbohydrates such as glycogen are formed, but also a large amount of energy rich carbon compounds is transferred into fat and lipids.

Biomass is the total mass of biological material.

DESCRIPTION OF THE FIGURES

FIG. 1. Schematic representation of plasmid pVDH275 harboring the neomycin-phosphotransferase gene (NPTII) flanked by the 35S cauliflower mosaic virus promoter (P35S) and terminator (T35S) as a selectable marker; an expression cassette comprising the pea plastocyanin promoter (pPCpea) and the nopaline synthase terminator (Tnos); right (RB) and left (LB) T-DNA border sequences and a bacterial kanamycin resistance (KanR) marker gene.

FIG. 2. Northern blot analysis of transgenic tobacco plants. Panel A depicts expression of otsA mRNA in leaves of individual pMOG799 transgenic tobacco plants. The control lane “C” contains total RNA from a non-transformed N. tabacum plant.

FIGS. 3A and 3B. Lineup of plant derived TPS encoding sequences compared with the TPS_(yeast) sequence using the Wisconsin GCG sequence analysis package (Devereux et al. (1984) A comprehensive set of sequence analysis programs of the VAX. Nucl. Acids Res., 12, 387).

FIG. 4. Alignment of PCR amplified tobacco TPS cDNA fragments with the TPS encoding yeast TPS1 gene. Boxes indicate identity between amino-acids of all four listed sequences.

FIG. 5. Alignment of PCR amplified tobacco TPP cDNA fragments with the TPP encoding yeast TPS2 gene. Boxes indicate identity between amino-acids of all four listed sequences.

FIG. 6. Alignment of a fragment of the PCR amplified sunflower TPS/TPP bipartite cDNA (SEQ ID NO: 24) with the TPP encoding yeast TPS2 gene. Boxes indicate identity between amino-acids of both sequences.

FIG. 7. Alignment of a fragment of the Arabidopsis TPS 1 and Rice EST clones with the TPS encoding yeast TPS 1 gene. Boxes indicate identity between amino-acids of all three sequences.

FIG. 8. Alignment of a fragment of the PCR amplified human TPS cDNA (SEQ ID NO: 10) with the TPS encoding yeast TPS1 gene. Boxes indicate identity between amino-acids of both sequences.

FIG. 9. Trehalose accumulation in tubers of pMOG1027 (35S astrehalase) transgenic potato plants.

FIG. 10. Hexokinase activity of a wild-type potato tuber (Solanum tuberosum cv. Kardal) extract with and without the addition of trehalose-6-phosphate.

FIG. 11. Hexokinase activity of a wild-type potato tuber (Solanum tuberosum cv. Kardal) extract with and without the addition of trehalose-6-phosphate. Frutose or glucose is used as a substrate for the assay.

FIG. 12. Hexokinase activity of a wild-type tobacco leaf extract (Nicotiana tabacum cv. SR1) with and without the addition of trehalose-6-phosphate. Fructose or glucose is used as substrate for the assay.

FIG. 13. Plot of a tobacco hexokinase activity measurement.

Data series 1: Tobacco plant extract Data series 2: Tobacco plant extract+1 mM trehalose-6-phosphate Data series 3: Commercial hexokinase extract from yeast (1/8 unit)

FIG. 14. Hexokinase activity of a wild-type rice leaf extract (Oryza sativa) extract with and without the addition of trehalose-6-phosphate. Experiments have been performed in duplicate using different amounts of extracts. Fructose or glucose is used as substrate for the assay.

FIG. 15. Hexokinase activity of a wild-type maize leaf extract (Zea mais) extract with and without the addition of trehalose-6-phosphate. Fructose or glucose is used as substrate for the assay.

FIG. 16. Fluorescence characteristics of wild-type (triangle), PC-TPS (square) and 35S-TPP (cross) tobacco leaves. The upper two panels show the electron transport efficiency (ETE) at the indicated light intensities (PAR). Plants were measured after a dark-period (upper-left panel) and after a light-period (upper-right panel). The bottom panels show reduction of fluorescence due to assimilate accumulation (non-photochemical quenching). Left and right panel as above.

FIG. 17. Relative sink-activity of plant-parts of PC-TPS (Famine) and 35S-TPP (Feast) transgenic tobacco plants. Indicated is the nett C-accumulation expressed as percentage of total C-content, for various plant-parts after a period of light (D) or light+dark (D+N).

FIG. 18. Actual distribution of carbon in plant-parts of PC-TPS (Famine) and 35S-TPP (Feast) transgenic tobacco plants. Indicated is the nett C-accumulation expressed as percentage of total daily accumulated new C for various plant-parts after a period of light (D) or light+dark (D+N).

FIG. 19. Scanned images showing reduced_and enchanced bolting in transgenic lettuce lines expressing PC-TPS or PC-TPP compared to wild-type plants. The lower panel shows leaf morphology and color.

FIGS. 20A-D. Profile of soluble sugars (FIGS. 20A and B) in extracts of transgenic lettuce (upper panel) and transgenic beet (lower panel) lines. In the upper pannel controls are GUS-trangenic lines which are compared to lines trangenics for PC-TPS and PC-TPP. In lower panel all transgenic are PC-TPS. Starch profiles are depicted in FIGS. 20B and C.

FIG. 21. Scanned image showing plant and leaf morphology of transgenic sugarbeet lines expressing PC-TPS (TPS) or PC-TPP (TPP) compared to wild-type plants (Control). TPS A-type has leaves which are comparable to wild-type while TPS D-type has clearly smaller leaves. The leaves of the TPP transgenic line have a lighter green color. A larger petiole and an increased size compared to the control.

FIG. 22. Taproot diameter of transgenic sugarbeet lines (PC-TPS). In the upper panel A, B, C and D indicate decreasing leaf sizes as compared to control (A). In the lower panel individual clones of control and PC-TPS line 286-2 are shown.

FIG. 23. Tuber yield of pMOG799 (35S TPS) transgenic potato lines.

FIG. 24. Tuber yield of pMOG1010 (35S TPP) and pMOG1124 (PC-TPP) transgenic potato lines.

FIG. 25. Tuber yield of 22 independent wild-type S. tuberosum clones.

FIG. 26. Tuber yield of pMOG1093 (PC-TPS) transgenic potato lines in comparison to wild-type. B, C, D, E, F, G indicate decreasing leaf sizes as compared to wild-type (B/C).

FIG. 27. Tuber yield of pMoG845 (Pat-TPS) transgenic potato lines (FIG. 27-1) in comparison to wild-type (FIG. 27-2). B, C indicate leaf sizes.

FIGS. 28A-C. Tuber yield of pMOG 1129 (845-11/22/28) transgenic potato lines.

FIGS. 29A-B. Scanned images showing cross section through leaves of TPP (FIG. 29B) and TPS (FIG. 29A) transgenic tobacco plants. Additional cell layers and increased cell size are visible in the TPS cross section.

FIG. 30. HPLC-PED analysis of tubers transgenic for TPS_(E.coli) before and after storage at 4° C. Kardal C, F, B, G and H are non-transgenic control lines.

FIG. 31. Scanned images showing leaf morphology, color and size of tobacco lines transgenic for 35S TPS (upper leaf), wild-type (middle leaf) and transgenic for 35S TPP (bottom leaf).

FIGS. 32A-D. Metabolic profiling of 35S TPS (pMOG799), 35S TPP (pMOG1010), wild-type (WT), PC-TPS (pMOG1177) and PC-TPP (pMOG1124) transgenic tobacco lines. Shown are the levels of trehalose, soluble sugars FIGS. 32A and B, starch and chlorophyll FIGS. 32C and D.

FIG. 33. Tuber yield of pMOG1027 (35S as-trehalase) and pMOG1027(845-11/22/28) (35S as-trehalase pat TPS) transgenic potato lines in comparison to wild-type potato lines.

FIG. 34. Starch content of pMOG1027 (35S as-trehalase) and pMOG1027 (845-11/22/28) (35S as-trehalase pat TPS) transgenic potato lines in comparison to wild-type potato lines. The sequence of all lines depicted is identical to FIG. 33.

FIGS. 35A-E. Yield of pMOG1028 (pat as-trehalase) and pMOG1028(845-11/22/28) (pat as-trehalase pat TPS) transgenic potato lines in comparison to wild-type potato lines.

FIG. 36. Yield of pMOG1092 (PC as-trehalase) transgenic potato lines in comparison to wild-type potato lines as depicted in FIGS. 35A-E.

FIG. 37. Yield of pMOG1130 (PC as-trehalase PC TPS) transgenic potato lines in comparison to wild-type potato lines as depicted in FIGS. 35A-E.

DETAILED DESCRIPTION OF THE INVENTION

The invention is concerned with the finding that metabolism can be modified in vivo by the level of T-6-P. A decrease of the intracellular concentration of T-6-P stimulates glycolytic activity. On the contrary, an increase of the T-6-P concentration will inhibit glycolytic activity and stimulate photosynthesis.

These modifications established by changes in T-6-P levels are most likely a result of the signalling function of hexokinase, which activity is shown to be regulated by T-6-P. An increase in the flux through hexokinase (i.e. an increase in the amount of glucose) that is reacted in glucose-6-phosphate has been shown to inhibit photosynthetic activity in plants. Furthermore, an increase in the flux through hexokinase would not only stimulate the glycolysis, but also cell division activity.

Theory of Trehalose-6-Phosphate Regulation of Carbon Metabolism

In a normal plant cell formation of carbohydrates takes place in the process of photosynthesis in which CO₂ is fixed and reduced to phosphorylated hexoses with sucrose as an end-product. Normally this sucrose is transported out of the cell to cells or tissues which through uptake of this sucrose can use the carbohydrates as building material for their metabolism or are able to store the carbohydrates as e.g. starch. In this respect, in plants, cells that are able to photosynthesize and thus to produce carbohydrates are denominated as sources, while cells which consume or store the carbohydrates are called sinks.

In animal and most microbial cells no photosynthesis takes place and the carbohydrates have to be obtained from external sources, either by direct uptake from saccharides (e.g. yeasts and other micro-organisms) or by digestion of carbohydrates (animals). Carbohydrate transport usually takes place in these organisms in the form of glucose, which is actively transported over the cell membrane.

After entrance into the cell, one of the first steps in the metabolic pathway is the phosphorylation of glucose into glucose-6-phosphate catalyzed by the enzyme hexokinase. It has been demonstrated that in plants sugars which are phosphorylated by hexokinase (HXK) are controlling the expression of genes involved in photosynthesis (Tang & Sheen (1994), The Plant Cell 6, 1665). Therefor, it has been proposed that HXK may have a dual function and may act as a key sensor and signal transmitter of carbohydrate-mediated regulation of gene-expression. It is believed that this regulation normally signals the cell about the availability of starting product, i.e. glucose. Similar effects are observed by the introduction of TPS or TPP which influence the level of T-6-P. Moreover, it is shown that in vitro T-6-P levels affect hexokinase activity. By increasing the level of T-6-P, the cell perceives a signal that there is a shortage of carbohydrate input. Conversely, a decrease in the level of T-6-P results in a signal that there is plenty of glucose, resulting in the down-regulation of photosynthesis: it signals that substrate for glycolysis and consequently energy supply for processes as cell growth and cell division is sufficiently available. This signalling is thought to be initiated by the increased flux through hexokinase (J. J. Van Oosten, public lecture at RijksUniversiteit Utrecht dated Apr. 19, 1996).

The theory that hexokinase signalling in plants can be regulated through modulation of the level of trehalose-6-phosphate would imply that all plants require the presence of an enzyme system able to generate and break-down the signal molecule trehalose-6-phosphate. Although trehalose is commonly found in a wide variety of fungi, bacterial, yeasts and algae, as well as in some invertebrates only a very limited range of vascular plants have been proposed to be able to synthesize this sugar (Elbein (1974), Adv. Carboh. Chem. Biochem. 30, 227). A phenomenon which was not understood until now is that despite the apparent lack of trehalose synthesizing enzymes, all plants do seem to contain trehalases, enzymes which are able to break down trehalose into two glucose molecules.

Indirect evidence for the presence of a metabolic pathway for trehalose is obtained by experiments presented herein with trehalase inhibitors such as Validamycin A or transformation with anti-sense trehalase.

Production of trehalose would be hampered if its intermediate T-6-P would influence metabolic activity too much. Preferably, in order to accumulate high levels of trehalose without affecting partitioning and allocation of metabolites by the action of trehalose-6-phosphate, one should overexpress a bipartite TPS/TPP enzyme. Such an enzyme would resemble a genetic constitution as found in yeast, where the TPS2 gene product harbours a TPS and TPP homologous region when compared with the E. coli otsA and otsB gene (Kaasen et al. (1994), Gene 145, 9). Using such an enzyme, trehalose-6-phosphate will not become freely available to other cell components. Another example of such a bipartite enzyme is given by Zentella & Iturriaga (Plant Physiol. (1996), 111 Abstract 88) who isolated a 3.2 kb cDNA from Selaginella lepidophylla encoding a putative trehalose-6-phosphate synthase/phosphatase. It is also envisaged that construction of a truncated TPS-TPP gene product, whereby only the TPS activity would be retained, would be as powerful for synthesis of T-6-P as the otsA gene of E. coli, also when used in homologous systems.

On a molecular level we have data that indicate that next to Selaginella also trehalose synthesizing genes are present in Arabidopsis, tobacco, rice and sunflower. Using degenerated primers, based on conserved sequences between TPS_(E.coli) and TPS_(yeast), we have been able to identify genes encoding putative trehalose-6-phosphate generating enzymes in sunflower and tobacco. Sequence comparison revealed significant homology between these sequences, the TPS genes from yeast and E. coli, and EST (expressed sequences tags) sequences from Arabidopsis and rice (see also Table 6b which contains the EST numbers of homologous EST's found).

Recently an Arabidopsis gene has been elucidated (disclosed in GENBANK Acc. No. Y08568, depicted in SEQ ID NO: 39) that on basis of its homology can be considered as a bipartite enzyme. These data indicate that, in contrast to current beliefs, most plants do contain genes which encode trehalose-phosphate-synthases enabling them to synthesize T-6-P. As proven by the accumulation of trehalose in TPS expressing plants, plants also contain phosphatases, non-specific or specific, able to dephosphorylate the T-6-P into trehalose. The presence of trehalase in all plants may be to effectuate turnover of trehalose.

Furthermore, we also provide data that T-6-P is involved in regulating carbohydrate pathways in human tissue. We have elucidated a human TPS gene (depicted in SEQ ID NO: 10) which shows homology with the TPS genes of yeast, E. coli and plants. Furthermore, we show data that also the activity of hexokinase is influenced in mammalian (mouse) tissue.

Generation of the “plenty” signal by decreasing the intracellular concentration of trehalose-6-phosphate through expression of the enzyme TPP (or inhibition of the enzyme TPS) will signal all cell systems to increase glycolytic carbon flow and inhibit photosynthesis. This is nicely shown in the experimental part, where, for instance in Experiment 2 transgenic tobacco plants are described in which the enzyme TPP is expressed having increased leaf size, increased branching and a reduction of the amount of chlorophyll. However, since the “plenty” signal is generated in the absence of sufficient supply of glucose, the pool of carbohydrates in the cell is rapidly depleted.

Thus, assuming that the artificial “plenty” signal holds on, the reduction in carbohydrates will finally become limiting for growth and cell division, i.e. the cells will use up all their storage carbohydrates and will be in a “hunger”-stage. Thus, leaves are formed with a low amount of stored carbohydrates. On the other hand, plants that express a construct with a gene coding for TPS, which increases the intracellular amount of T-6-P, showed a reduction of leaf size, while also the leaves were darker green, and contained an increased amount of chlorophyll.

In yeast, a major role of glucose-induced signalling is to switch metabolism from a neogenetic/respirative mode to a fermentative mode. Several signalling pathways are involved in this phenomenon (Thevelein and Hohmann, (1995) TIBS 20, 3). Besides the possible role of hexokinase signalling, the RAS-cyclic-AMP (cAMP) pathway has been shown to be activated by glucose. Activation of the RAS-cAMP pathway by glucose requires glucose phosphorylation, but no further glucose metabolism. So far, this pathway has been shown to activate trehalase and 6-phosphofructo-2-kinase (thereby stimulating glycolysis), while fructose-1,6-bisphosphatase is inhibited (thereby preventing gluconeogenesis), by cAMP-dependent protein phosphorylation. This signal transduction route and the metabolic effects it can bring about can thus be envisaged as one that acts in parallels with the hexokinase signalling pathway, that is shown to be influenced by the level of trehalose-6-phosphate.

As described in our invention, transgenic plants expressing as-trehalase reveal similar phenomena, like dark-green leaves, enhanced yield, as observed when expressing a TPS gene. It also seems that expression of as-trehalase in double-constructs enhances the effects that are caused by the expression of TPS. Trehalase activity has been shown to be present in e.g. plants, insects, animals, fungi and bacteria while only in a limited number of species, trehalose is accumulated.

Up to now, the role of trehalase in plants is unknown although this enzyme is present in almost all plant-species. It has been proposed to be involved in plant pathogen interactions and/or plant defense responses. We have isolated a potato trehalase gene and show that inhibition of trehalase activity in potato leaf and tuber tissues leads to an increase in tuber-yield. Fruit-specific expression of as-trehalase in tomato combined with TPS expression dramatically alters fruit development.

According to one embodiment of the invention, accumulation of T-6-P is brought about in cells in which the capacity of producing T-6-P has been introduced by introduction of an expressible gene construct encoding trehalose-phosphate-synthase (TPS). Any trehalose phosphate synthase gene under the control of regulatory elements necessary for expression of DNA in cells, either specifically or constitutively, may be used, as long as it is capable of producing a trehalose phosphate synthase capable of T-6-P production in said cells. One example of an open reading frame according to the invention is one encoding a TPS-enzyme as represented in SEQ ID NO: 2. Other examples are the open reading frames as represented in SEQ ID NO's: 10, 18-23, 41 and 45-53. As is illustrated by the above-mentioned sequences it is well known that more than one DNA sequence may encode an identical enzyme, which fact is caused by the degeneracy of the genetic code. If desired, the open reading frame encoding the trehalose phosphate synthase activity may be adapted to codon usage in the host of choice, but this is not a requirement.

The isolated nucleic acid sequence represented by for instance SEQ ID NO: 2, may be used to identify trehalose phosphate synthase genes in other organisms and subsequently isolating and cloning them, by PCR techniques and/or by hybridizing DNA from other sources with a DNA- or RNA fragment obtainable from the E. coli gene. Preferably, such DNA sequences are screened by hybridizing under more or less stringent conditions (influenced by factors such as temperature and ionic strength of the hybridization mixture). Whether or not conditions are stringent also depends on the nature of the hybridization, i.e. DNA:DNA, DNA:RNA, RNA:RNA, as well as the length of the shortest hybridizing fragment. Those of skill in the art are readily capable of establishing a hybridization regime stringent enough to isolate TPS genes, while avoiding non-specific hybridization. As genes involved in trehalose synthesis from other sources become available these can be used in a similar way to obtain an expressible trehalose phosphate synthase gene according to the invention. More detail is given in the experimental section.

Sources for isolating trehalose phosphate synthase activities include microorganisms (e.g. bacteria, yeast, fungi), plants, animals, and the like. Isolated DNA sequences encoding trehalose phosphate synthase activity from other sources may be used likewise in a method for producing T-6-P according to the invention. As an example, genes for producing T-6-P from yeast are disclosed in WO 93/17093.

The invention also encompasses nucleic acid sequences which have been obtained by modifying the nucleic acid sequence represented in SEQ ID NO: 1 by mutating one or more codons so that it results in amino acid changes in the encoded protein, as long as mutation of the amino acid sequence does not entirely abolish trehalose phosphate synthase activity.

According to another embodiment of the invention the trehalose-6-phosphate in a cell can be converted into trehalose by trehalose phosphate phosphatase encoding genes under control of regulatory elements necessary for the expression of DNA in cells. A preferred open reading frame according to the invention is one encoding a TPP-enzyme as represented in SEQ ID NO: 4 (Kaasen et al. (1994) Gene, 145, 9). It is well known that more than one DNA sequence may encode an identical enzyme, which fact is caused by the degeneracy of the genetic code. If desired, the open reading frame encoding the trehalose phosphate phosphatase activity may be adapted to codon usage in the host of choice, but this is not a requirement.

The isolated nucleic acid sequence represented by SEQ ID NO: 3, may be used to identify trehalose phosphate phosphatase genes in other organisms and subsequently isolating and cloning them, by PCR techniques and/or by hybridizing DNA from other sources with a DNA- or RNA fragment obtainable from the E. coli gene. Preferably, such DNA sequences are screened by hybridizing under more or less stringent conditions (influenced by factors such as temperature and ionic strength of the hybridization mixture). Whether or not conditions are stringent also depends on the nature of the hybridization, i.e. DNA:DNA, DNA:RNA, RNA:RNA, as well as the length of the shortest hybridizing fragment. Those of skill in the art are readily capable of establishing a hybridization regime stringent enough to isolate TPP genes, while avoiding aspecific hybridization. As genes involved in trehalose synthesis from other sources become available these can be used in a similar way to obtain an expressible trehalose phosphate phosphatase gene according to the invention. More detail is given in the experimental section.

Sources for isolating trehalose phosphate phosphatase activities include microorganisms (e.g. bacteria, yeast, fungi), plants, animals, and the like. Isolated DNA sequences encoding trehalose phosphate phosphatase activity from other sources may be used likewise.

The invention also encompasses nucleic acid sequences which have been obtained by modifying the nucleic acid sequence represented in SEQ ID NO: 3 by mutating one or more codons so that it results in amino acid changes in the encoded protein, as long as mutation of the amino acid sequence does not entirely abolish trehalose phosphate phosphatase activity.

Other enzymes with TPS or TPP activity are represented by the so-called bipartite enzymes. It is envisaged that the part of the sequence which is specifically coding for one of the two activities can be separated from the part of the bipartite enzyme coding for the other activity. One way to separate the activities is to insert a mutation in the sequence coding for the activity that is not selected, by which mutation the expressed protein is impaired or deficient of this activity and thus only performs the other function. This can be done both for the TPS- and TPP-activity coding sequence. Thus, the coding sequences obtained in such a way can be used for the formation of novel chimaeric open reading frames capable of expression of enzymes having either TPS or TPP activity.

According to another embodiment of the invention, especially plants can be genetically altered to produce and accumulate the above-mentioned enzymes in specific parts of the plant. Preferred sites of enzyme expression are leaves and storage parts of plants. In particular potato tubers are considered to be suitable plant parts. A preferred promoter to achieve selective TPS-enzyme expression in microtubers and tubers of potato is obtainable from the region upstream of the open reading frame of the patatin gene of potato.

Another suitable promoter for specific expression is the plastocyanin promoter, which is specific for photoassimilating parts of plants. Furthermore, it is envisaged that specific expression in plant parts can yield a favourable effect for plant growth and reproduction or for economic use of said plants. Promoters which are useful in this respect are: the E8-promoter (EP 0 409 629) and the 2A11-promoter (van Haaren and Houck (1993), Plant Mol. Biol., 221, 625) which are fruit-specific; the cruciferin promoter, the napin promoter and the ACP promoter which are seed-specific; the PAL-promoter; the chalcon-isomerase promoter which is flower-specific; the SSU promoter, and ferredoxin promoter, which are leaf-specific; the TobRb7 promoter which is root-specific, the RolC promoter which is specific for phloem and the HMG2 promoter (Enjuto et al. (1995). Plant Cell 7, 517) and the rice PCNA promoter (Kosugi et al. (1995), Plant J. 7, 877) which are specific for meristematic tissue.

Another option under this invention is to use inducible promoters. Promoters are known which are inducible by pathogens, by stress, by chemical or light/dark stimuli. It is envisaged that for induction of specific phenoma, for instance sprouting, bolting, seed setting, filling of storage tissues, it is beneficial to induce the activity of the genes of the invention by external stimuli. This enables normal development of the plant and the advantages of the inducibility of the desired phenomena at control. Promoters which qualify for use in such a regime are the pathogen inducible promoters described in DE 4446342 (fungus and auxin inducible PRP-1), WO 96/28561 (fungus inducible PRP-1), EP 0 586 612 (nematode inducible), EP 0 712 273 (nematode inducible), WO 96/34949 (fungus inducible), PCT/EP96/02437 (nematode inducible), EP 0 330 479 (stress inducible), U.S. Pat. No. 5,510,474 (stress inducible), WO 96/12814 (cold inducible), EP 0 494 724 (tetracycline inducible), EP 0 619 844 (ethylene inducible), EP 0 337 532 (salicylic acid inducible), WO 95/24491 (thiamine inducible) and WO 92/19724 (light inducible). Other chemical inducible promoters are described in EP 0 674 608, EP 637 339, EP 455 667 and U.S. Pat. No. 5,364,780.

According to another embodiment of the invention, cells are transformed with constructs which inhibit the function of the endogenously expressed TPS or TPP. Inhibition of undesired endogenous enzyme activity is achieved in a number of ways, the choice of which is not critical to the invention. One method of inhibition of gene expression is achieved through the so-called ‘antisense approach.’ Herein a DNA sequence is expressed which produces an RNA that is at least partially complementary to the RNA which encodes the enzymatic activity that is to be blocked. It is preferred to use homologous antisense genes as these are more efficient than heterologous genes.

An alternative method to block the synthesis of undesired enzymatic activities is the introduction into the genome of the plant host of an additional copy of an endogenous gene present in the plant host. It is often observed that such an additional copy of a gene silences the endogenous gene: this effect is referred to in the literature as the co-suppressive effect, or co-suppression. Details of the procedure of enhancing substrate availability are provided in the Examples of WO 95/01446, incorporated by reference herein.

Host cells can be any cells in which the modification of hexokinase-signalling can be achieved through alterations in the level of T-6-P. Thus, accordingly, all eukaryotic cells are subject to this invention. From an economic point of view the cells most suited for production of metabolic compounds are most suitable for the invention. These organisms are, amongst others, plants animals, yeast, fungi. However, also expression in specialized animal cells (like pancreatic beta-cells and fat cells) is envisaged.

Preferred plant hosts among the Spermatophytae are the Angiospermae, notably the Dicotyledoneae, comprising inter alia the Solanaceae as a representative family, and the Monocotyledoneae, comprising inter alia the Gramineae as a representative family. Suitable host plants, as defined in the context of the present invention include plants (as well as parts and cells of said plants) and their progeny which contain a modified level of T-6-P, for instance by using recombinant DNA techniques to cause or enhance production of TPS or TPP in the desired plant or plant organ. Crops according to the invention include those which have flowers such as cauliflower (Brassica oleracea), artichoke (Cynara scolymus), cut flowers like carnation (Dianthus caryophyllus), rose (Rosa spp), Chrysanthemum, Petunia, Alstromeria, Gerbera, Gladiolus, lily (Lilium spp), hop (Humulus lupulus), broccoli, potted plants like Rhododendron, Azalia, Dahlia, Begonia, Fuchsia, Geranium etc.; fruits such as apple (Malus, e.g. domesticus), banana (Musa, e.g. Acuminata), apricot (Prunus armeniaca), olive (Oliva sativa), pineapple (Ananas comosus), coconut (Cocos nucifera), mango (Mangifera indica), kiwi, avocado (Persea americana), berries (such as the currant, Ribes, e.g. rubrum), cherries (such as the sweet cherry, Prunus, e.g. avium), cucumber (Cucumis, e.g. sativus), grape (Vitis, e.g. vinifera), lemon (Citrus limon), melon (Cucumis melo), mustard (Sinapis alba and Brassica nigra), nuts (such as the walnut, Juglans, e.g. regia; peanut, Arachis hypogeae), orange (Citrus, e.g. maxima), peach (Prunus, e.g. persica), pear (Pyra, e.g. Communis), pepper (Solanum, e.g. capsicum), plum (Prunus, e.g. domestica), strawberry (Fragaria, e.g. moschata), tomato (Lycopersicon, e.g. esculentum); leaves, such as alfalfa (Medicago sativa), cabbages (such as Brassica oleracea), endive (Cichoreum, e.g. endivia), leek (Allium porruin), lettuce (Lactuca sativa), spinach (Spinacia oleraceae), tobacco (Nicociana tabacum), grasses like Festuca, Poa, rye-grass (such as Lolium perenne, Lolium multiflorum and Arrenatherum spp.), amenity grass, turf, seaweed, chicory (Cichorium intybus), tea (Thea sinensis), celery, parsley (Pecroselinum crispum), chevil and other herbs; roots, such as arrowroot (Maranta arundinacea), beet (Beta vulgaris), carrot (Daucus carota), cassaya (Manihot esculenta), ginseng (Panax ginseng), turnip (Brassica rapa), radish (Raphanus sativus), yam (Dioscorea esculenta), sweet potato (Ipomoea batatas), taro; seeds, such as beans (Phaseolus vulgaris), pea (Pisum sativum), soybean (Glycin max), wheat (Triticum aestivum), barley (Hordeum vulgare), corn (Zea mays), rice (Oryza sativa), bush beans and broad beans (Vicia faba), cotton (Gossypium spp.), coffee (Coffea arabica and C. canephora); tubers, such as kohlrabi (Brassica oleraceae), potato (Solanum tuberosum); bulbous plants as onion (Allium cepa), scallion, tulip (Tulipa spp.), daffodil (Narcissus spp.), garlic (Allium sativum); stems such as cork-oak, sugarcane (Saccharum spp.), sisal (Sisal spp.), flax (Linum vulgare), jute; trees like rubber tree, oak (Quercus spp.), beech (Betula spp.), alder (Alnus spp.), ashtree (Acer spp.), elm (Ulmus spp.), palms, ferns, ivies and the like.

Transformation of yeast and fungal or animal cells can be done through normal state-of-the art transformation techniques through commonly known vector systems like pBluescript, pUC and viral vector systems like RSV and SV40.

The method of introducing the expressible trehalose-phosphate synthase gene, the expressible trehalose-phosphate-phosphatase gene, or any other sense or antisense gene into a recipient plant cell is not crucial, as long as the gene is expressed in said plant cell.

Although some of the embodiments of the invention may not be practicable at present, e.g. because some plant species are as yet recalcitrant to genetic transformation, the practicing of the invention in such plant species is merely a matter of time and not a matter of principle, because the amenability to genetic transformation as such is of no relevance to the underlying embodiment of the invention.

Transformation of plant species is now routine for an impressive number of plant species, including both the Dicotyledoneae as well as the Monococyledoneae. In principle any transformation method may be used to introduce chimeric DNA according to the invention into a suitable ancestor cell. Methods may suitably be selected from the calcium/polyethylene glycol method for protoplasts (Krens et al. (1982), Nature 296, 72; Negrutiu et al. (1987), Plant Mol. Biol. 8, 363, electroporation of protoplasts (Shillito et al. (1985) Bio/Technol. 3, 1099), microinjection into plant material (Crossway et al. (1986), Mol. Gen. Genet. 202), (DNA or RNA-coated) particle bombardment of various plant material (Klein at al. (1987), Nature 327, 70), infection with (non-integrative) viruses, in planta Agrobacterium tumefaciens mediated gene transfer by infiltration of adult plants or transformation of mature pollen or microspores (EP 0 301 316) and the like. A preferred method according to the invention comprises Agrobacterium-mediated DNA transfer. Especially preferred is the use of the so-called binary vector technology as disclosed in EP A 120 516 and U.S. Pat. No. 4,940,838).

Although considered somewhat more recalcitrant towards genetic transformation, monocotyledonous plants are amenable to transformation and fertile transgenic plants can be regenerated from transformed cells or embryos, or other plant material. Presently, preferred methods for transformation of monocots are microprojectile bombardment of embryos, explants or suspension cells, and direct DNA uptake or (tissue) electroporation (Shimamoto et al. (1989), Nature 338, 274-276). Transgenic maize plants have been obtained by introducing the Screptomyces hygroscopicus bar-gene, which encodes phosphinothricin acetyltransferase (an enzyme which inactivates the herbicide phosphinothricin), into embryogenic cells of a maize suspension culture by microprojectile bombardment (Gordon-Kamm (1990), Plant Cell, 2, 603). The introduction of genetic material into aleurone protoplasts of other monocot crops such as wheat and barley has been reported (Lee (1989), Plant Mol. Biol. 13, 21). Wheat plants have been regenerated from embryogenic suspension culture by selecting embryogenic callus for the establishment of the embryogenic suspension cultures (Vasil (1990) Bio/Technol. 8, 429). The combination with transformation systems for these crops enables the application of the present invention to monocots.

Monocotyledonous plants, including commercially important crops such as rice and corn are also amenable to DNA transfer by Agrobacterium strains (vide WO 94/00977, EP 0 159 418 B1; Gould et al. (1991) Plant. Physiol. 95, 426-434).

To obtain transgenic plants capable of constitutively expressing more than one chimeric gene, a number of alternatives are available including the following:

A. The use of DNA, e.g a T-DNA on a binary plasmid, with a number of modified genes physically coupled to a second selectable marker gene. The advantage of this method is that the chimeric genes are physically coupled and therefore migrate as a single Mendelian locus. B. Cross-pollination of transgenic plants each already capable of expressing one or more chimeric genes, preferably coupled to a selectable marker gene, with pollen from a transgenic plant which contains one or more chimeric genes coupled to another selectable marker. Afterwards the seed, which is obtained by this crossing, maybe selected on the basis of the presence of the two selectable markers, or on the basis of the presence of the chimeric genes themselves. The plants obtained from the selected seeds can afterwards be used for further crossing. In principle the chimeric genes are not on a single locus and the genes may therefore segregate as independent loci. C. The use of a number of a plurality chimeric DNA molecules, e.g. plasmids, each having one or more chimeric genes and a selectable marker. If the frequency of co-transformation is high, then selection on the basis of only one marker is sufficient. In other cases, the selection on the basis of more than one marker is preferred. D. Consecutive transformation of transgenic plants already containing a first, second, (etc), chimeric gene with new chimeric DNA, optionally comprising a selectable marker gene. As in method B, the chimeric genes are in principle not on a single locus and the chimeric genes may therefore segregate as independent loci. E. Combinations of the above mentioned strategies.

The actual strategy may depend on several considerations as maybe easily determined such as the purpose of the parental lines (direct growing, use in a breeding programme, use to produce hybrids) but is not critical with respect to the described invention.

It is known that practically all plants can be regenerated from cultured cells or tissues. The means for regeneration vary from species to species of plants, but generally a suspension of transformed protoplasts or a petri plate containing transformed explants is first provided. Shoots may be induced directly, or indirectly from callus via organogenesis or embryogenesis and subsequently rooted. Next to the selectable marker, the culture media will generally contain various amino acids and hormones, such as auxin and cytokinins. It is also advantageous to add glutamic acid and proline to the medium, especially for such species as corn and alfalfa. Efficient regeneration will depend on the medium, on the genotype and on the history of the culture. If these three variables are controlled regeneration is usually reproducible and repeatable. After stable incorporation of the transformed gene sequences into the transgenic plants, the traits conferred by them can be transferred to other plants by sexual crossing. Any of a number of standard breeding techniques can be used, depending upon the species to be crossed.

Suitable DNA sequences for control of expression of the plant expressible genes (including marker genes), such as transcriptional initiation regions, enhancers, non-transcribed leaders and the like, may be derived from any gene that is expressed in a plant cell. Also intended are hybrid promoters combining functional portions of various promoters, or synthetic equivalents thereof. Apart from constitutive promoters, inducible promoters, or promoters otherwise regulated in their expression pattern, e.g. developmentally or cell-type specific, may be used to control expression of the expressible genes according to the invention.

To select or screen for transformed cells, it is preferred to include a marker gene linked to the plant expressible gene according to the invention to be transferred to a plant cell. The choice of a suitable marker gene in plant transformation is well within the scope of the average skilled worker; some examples of routinely used marker genes are the neomycin phosphotransferase genes conferring resistance to kanamycin (EP-B 131 623), the glutathion-S-transferase gene from rat liver conferring resistance to glutathione derived herbicides (EP-A 256 223), glutamine synthetase conferring upon overexpression resistance to glutamine synthetase inhibitors such as phosphinothricin (WO 87/05327), the acetyl transferase gene from Streptomyces viridochromogenes conferring resistance to the selective agent phosphinothricin (EP-A 275 957), the gene encoding a 5-enolshikimate-3-phosphate synthase (EPSPS) conferring tolerance to N-phosphonomethylglycine, the bar gene conferring resistance against Bialaphos (e.g. WO 91/02071) and the like. The actual choice of the marker is not crucial as long as it is functional (i.e. selective) in combination with the plant cells of choice.

The marker gene and the gene of interest do not have to be linked, since co-transformation of unlinked genes (U.S. Pat. No. 4,399,216) is also an efficient process in plant transformation.

Preferred plant material for transformation, especially for dicotyledonous crops are leaf-discs which can be readily transformed and have good regenerative capability (Horsch et al. (1985), Science 227, 1229).

Specific use of the invention is envisaged in the following ways: as can be seen from the Examples the effects of the expression of TPP (which causes a decrease in the intracellular T-6-P concentration) are an increased leaf size, increased branching leading t6 an increase in the number of leaves, increase in total leaf biomass, bleaching of mature leaves, formation of more small flowers and sterility. These effects are specifically useful in the following cases: increased leaf size (and increase in the number of leaves) is economically important for leafy vegetables such as spinach, lettuce, leek, alfalfa, silage maize; for ground coverage and weed control by grasses and garden plants; for crops in which the leaves are used as product, such as tobacco, tea, hemp and roses (perfumes!); for the matting up of cabbage-like crops such as cauliflower.

An additional advantage of the fact that these leaves are stimulated in their metabolic activity is that they tend to burn all their intracellular resources, which means that they are low in starch-content. For plants meant for consumption a reduction in starch content is advantageous in the light of the present tendency for low-calorie foodstuffs. Such a reduction in starch content also has effects on taste and texture of the leaves. An increase in the protein/carbohydrate balance as can be produced by the expression of TPP is especially important for leafy crops as silage maize.

Increased branching, which is accompanied by a tendency to have stems with a larger diameter, can be advantageous in crops in which the stem is responsible for the generation of an economically attractive product. Examples in this category are all trees for the increased production of wood, which is also a starting material for paper production; crops like hemp, sisal, flax which are used for the production of rope and linen; crops like bamboo and sugarcane; rubber-tree, cork-oak; for the prevention of flattening in crops or crop parts, like grains, corn, legumes and strawberries.

A third phenomenon is increased bleaching of the leaves (caused by a decrease of photosynthetic activity). Less colorful leaves are preferred for crops such as chicory and asparagus. Also for cut flowers bleaching in the petals can be desired, for instance in Alstromeria.

An overall effect is the increase in biomass resulting from an increase in metabolic activity. This means that the biomass consists of metabolized compounds such as proteins and fats. Accordingly, there is an increased protein/carbohydrate balance in mature leaves which is an advantage for crops like silage maize, and all fodder which can be ensilaged. A similar increased protein/carbohydrate balance can be established in fruits, tubers and other edible plant parts.

Outside the plant kingdom an increased metabolism would be beneficial for protein production in microorganisms or eukaryotic cell cultures. Both production of endogenous but also of heterologous proteins will be enhanced which means that the production of heterologous proteins in cultures of yeast or other unicellular organisms can be enhanced in this way. For yeast this would give a more efficient fermentation, which would result in an increased alcohol yield, which of course is favourable in brewery processes, alcohol production and the like.

In animals or human beings it is envisaged that diseases caused by a defect in metabolism can be overcome by stable expression of TPP or TPS in the affected cells. In human cells, the increased glucose consumption of many tumour cells depends to a large extent on the overexpression of hexokinase (Rempel et al. (1996) FEBS Lett. 385, 233). It is envisaged that the flux of glucose into the metabolism of cancer cells can be influenced by the expression of trehalose-6-phosphate synthesizing enzymes. It has also been shown that the hexokinase activation is potentiated by the cAMP/PKA (protein kinase A pathway). Therefore, inactivation of this signal transduction pathway may affect glucose uptake and the proliferation of neoplasias. Enzyme activities in mammalian cells able to synthesize trehalose-6-phosphate and trehalose and degrade trehalose have been shown in e.g. rabbit kidney cortex cells (Sacktor (1968) Proc. Natl. Acad. Sci. USA 60, 1007).

Another example can be found in defects in insulin secretion in pancreatic beta-cells in which the production of glucose-6-phosphate catalyzed by hexokinase is the predominant reaction that couples rises in extracellular glucose levels to insulin secretion (Efrat et al. (1994), TIBS 19, 535). An increase in hexokinase activity caused by a decrease of intracellular T-6-P then will stimulate insulin production in cells which are deficient in insulin secretion.

Also in transgenic animals an increased protein/carbohydrate balance can be advantageous. Both the properties of on increased metabolism and an enhanced production of proteins are of large importance in farming in which animals should gain in flesh as soon as possible. Transformation of the enzyme TPP into meat-producing animals like chickens, cattle, sheep, turkeys, goats, fish, lobster, crab, shrimps, snails etc, will yield animals that grow faster and have a more proteinaceous meat.

In the same way this increased metabolism means an increase in the burn rate of carbohydrates and it thus prevents obesity.

More plant-specific effects from the decrease of intracellular T-6-P concentration are an increase in the number of flowers (although they do not seem to lead to the formation of seed). However, an increase in the number of flowers is advantageous for cutflower plants and pot flower plants and also for all plants suitable for horticulture.

A further effect of this flowering phenomenon is sterility, because the plants do not produce seed. Sterile plants are advantageous in hybrid breeding.

Another economically important aspect is the prohibiting of bolting of culture crops such as lettuce, endive and both recreational and fodder grasses. This is a beneficial property because it enables the crop to grow without having to spend metabolic efforts to flowering and seed production. Moreover, in crops like lettuce, endive and grasses the commercial product/application is non-bolted.

Specific expression of TPP in certain parts (sinks) of the plant can give additional beneficial effects. It is envisaged that expression of TPP by a promoter which is active early in e.g. seed forming enables an increased growth of the developing seed. A similar effect would be obtained by expressing TPP by a flower-specific promoter. To put it shortly: excessive growth of a certain plant part is possible if TPP is expressed by a suitable specific promoter. In fruits specific expression can lead to an increased growth of the skin in relation to the flesh. This enables improvement of the peeling of the fruit, which can be advantageous for automatic peeling industries.

Expression of TPP during the process of germination of oil-storing seeds prevents oil-degradations. In the process of germination, the glyoxylate cycle is very active. This metabolic pathway converts acetyl-CoA via malate into sucrose which can be transported and used as energy source during growth of the seedling. Key-enzymes in this process are malate synthase and isocitrate lyase. Expression of both enzymes is supposed to be regulated by hexokinase signalling. One of the indications for this regulation is that both 2-deoxyglucose and mannose are phosphorylated by hexokinase and able to transduce their signal, being reduction of malate synthase and isocitrate lyase expression, without being further metabolised. Expression of TPP in the seed, thereby decreasing the inhibition of hexokinase, thereby inhibiting malate synthase and isocitrate lyase maintains the storage of oil into the seeds and prevents germination.

In contrast to the effects of TPP the increase in T-6-P caused by the expression of TPS causes other effects as is illustrated in the Examples. From these it can be learnt that an increase in the amount of T-6-P causes dwarfing or stunted growth (especially at high expression of TPS), formation of more lancet-shaped leaves, darker color due to an increase in chlorophyll and an increase in starch content. As is already acknowledged above, the introduction of an anti-sense trehalase construct will also stimulate similar effects as the introduction of TPS. Therefore, the applications which are shown or indicated for TPS will equally be established by using as-trehalase. Moreover, the use of double-constructs of TPS and as-trehalase enhances the effects of a single construct.

Dwarfing is a phenomenon that is desired in horticultural plants, of which the Japanese bonsai trees are a proverbial example. However, also creation of mini-flowers in plants like allseed, roses, Amaryllis, Hortensia, birch and palm will have economic opportunities. Next to the plant kingdom dwarfing is also desired in animals. It is also possible to induce bolting in culture crops such as lettuce. This is beneficial because it enables a rapid production of seed. Ideally the expression of TPS for this effect should be under control of an inducible promoter.

Loss of apical dominance also causes formation of multiple shoots which is of economic importance for instance in alfalfa.

A reduction in growth is furthermore desired for the industry of “veggie snacks”, in which vegetables are considered to be consumed in the form of snacks. Chemy-tomatoes is an example of reduced size vegetables which are successful in the market. It can be envisaged that also other vegetables like cabbages, cauliflower, carrot, beet and sweet potato and fruits like apple, pear, peach, melon, and several tropical fruits like mango and banana would be marketable on miniature size.

Reduced growth is desired for all cells that are detrimental to an organism, such as cells of pathogens and cancerous cells. In this last respect a role can be seen in regulation of the growth by changing the level of T-6-P. An increase in the T-6-P level would reduce growth and metabolism of cancer tissue. One way to increase the intracellular level of T-6-P is to knock-out the TPP gene of such cells by introducing a specific recombination event which causes the introduction of a mutation in the endogenous TPP-genes. One way in which this could be done is the introduction of a DNA-sequence able of introducing a mutation in the endogenous gene via a cancer cell specific internalizing antibody. Another way is targeted microparticle bombardment with said DNA. Thirdly a cancer cell specific viral vectors having said DNA can be used.

The phenomenon of a darker green color seen with an increased concentration of T-6-P, is a property which is desirable for pot flower plants and, in general, for species in horticulture and for recreational grasses.

Increase in the level of T-6-P also causes an increase in the storage carbohydrates such as starch and sucrose. This then would mean that tissues in which carbohydrates are stored would be able to store more material. This can be illustrated by the Examples where it is shown that in plants increased biomass of storage organs such as tubers and thickened roots as in beets (storage of sucrose) are formed.

Crops in which this would be very advantageous are potato, sugarbeet, carrot, chicory and sugarcane.

An additional economically important effect in potatoes is that after transformation with DNA encoding for the TPS gene (generating an increase in T-6-P) it has been found that the amount of soluble sugars decreases, even after harvest and storage of the tubers under cold conditions (4° C.). Normally even colder storage would be necessary to prevent early sprouting, but this results in excessive sweetening of the potatoes. Reduction of the amount of reducing sugars is of major importance for the food industry since sweetened potato tuber material is not suitable for processing because a Maillard reaction will take place between the reducing sugars and the amino-acids which results in browning.

In the same way also inhibition of activity of invertase can be obtained by transforming sugarbeets with a polynucleotide encoding for the enzyme TPS. Inhibition of invertase activity in sugarbeets after harvest is economically very important.

Also in fruits and seeds, storage can be altered. This does not only result in an increased storage capacity but in a change in the composition of the stored compounds. Crops in which improvements in yield in seed are especially important are maize, rice, cereals, pea, oilseed rape, sunflower, soybean and legumes. Furthermore, all fruitbearing plants are important for the application of developing a change in the amount and composition of stored carbohydrates. Especially for fruit the composition of stored products gives changes in solidity and firmness, which is especially important in soft fruits like tomato, banana, strawberry, peach, berries and grapes.

In contrast to the effects seen with the expression of TPP, the expression of TPS reduces the ratio of protein/carbohydrate in leaves. This effect is of importance in leafy crops such as fodder grasses and alfalfa. Furthermore, the leaves have a reduced biomass, which can be of importance in amenity grasses, but, more important, they have a relatively increased energy content. This property is especially beneficial for crops as onion, leek and silage maize.

Furthermore, also the viability of the seeds can be influenced by the level of intracellularly available T-6-P.

Combinations of expression of TPP in one part of a plant and TPS in an other part of the plant can synergize to increase the above-described effects. It is also possible to express the genes sequential during development by using specific promoters. Lastly, it is also possible to induce expression of either of the genes involved by placing the coding the sequence under control of an inducible promoter. It is envisaged that combinations of the methods of application as described will be apparent to the person skilled in the art.

The invention is further illustrated by the following examples. It is stressed that the Examples show specific embodiments of the inventions, but that it will be clear that variations on these examples and use of other plants or expression systems are covered by the invention.

EXPERIMENTAL DNA Manipulations

All DNA procedures (DNA isolation from E. coli, restriction, ligation, transformation, etc.) are performed according to standard protocols (Sambrook et al. (1989) Molecular Cloning: a laboratory manual, 2nd ed. Cold Spring Harbor Laboratory Press, CSH, New York).

Strains

In all examples E. coli K-12 strain DH5a is used for cloning. The Agrobacterium tumefaciens strains used for plant transformation experiments are EHA 105 and MOG 101 (Hood et al. (1993) Trans. Research 2, 208).

Construction of Agrobacterium Strain MOG101 Construction of Agrobacterium strain MOG101 is described in WO 96/21030. Cloning of the E. Coli otsA Gene and Construction of pMOG799

In E. coli trehalose phosphate synthase (TPS) is encoded by the otsA gene located in the operon otsBA. The cloning and sequence determination of the otsA gene is described in detail in Example I of WO95/01446, herein incorporated by reference. To effectuate its expression in plant cells, the open reading frame has been linked to the transcriptional regulatory elements of the CaMV 35S RNA promoter, the translational enhancer of the ALMV leader, and the transcriptional terminator of the nos-gene, as described in greater detail in Example I of WO95/01446, resulting in pMOG799. A sample of an E. coli strain harboring pMOG799 has been deposited under the Budapest Treaty at the Centraal Bureau voor Schimmelcultures, Oosterstraat 1, P.O. Box 273, 3740 AG Baarn, The Netherlands, on Monday 23 Aug. 1993: the Accession Number given by the International Depositary Institution is CBS 430.93.

Isolation of a Patatin Promoter/Construction of pMOG546

A patatin promoter fragment is isolated from chromosomal DNA of Solanum _(—) tuberosum cv. Bintje using the polymerase chain reaction. A set of oligonucleotides, complementary to the sequence of the upstream region of Apat21 patatin gene (Bevan et al. (1986) Nucl. Acids Res. 14, 5564), is synthesized consisting of the following sequences:

(SEQ ID NO: 5) 5′ AAG CTT ATG TTG CCA TAT AGA GTA G 3′ PatB33.2 (SEQ ID NO: 6) 5′ GTA GTT GCC ATG GTG CAA ATG TTC 3′ PatATG.2

These primers are used to PCR amplify a DNA fragment of 1123 bp, using chromosomal DNA isolated from potato cv. Bintje as a template. The amplified fragment shows a high degree of similarity to the Apat21 patatin sequence and is cloned using EcoRI linkers into a pUC18 vector resulting in plasmid pMOG546.

Construction of pMOG845

Construction of pMOG845 is described in WO 96/21030.

Construction of pVDH318, Plastocvanin-TPS

Plasmid pMOG79B (described in WO95/01446) is digested with HindIII and ligated with the oligonucleotide duplex TCV11 and TCV12 (see construction of pMOG845). The resulting vector is digested with PstI and HindIII followed by the insertion of the PotPiII terminator resulting in pTCV118. Plasmid pTCV118 is digested with SmaI and HindIII yielding a DNA fragment comprising the TPS coding region and the PotPiII terminator. BglII linkers were added and the resulting fragment was inserted in the plant binary expression vector pVDH275 (FIG. 1) digested with BamHI, yielding pVDH318. pVDH275 is a derivative of pMOG23 (Sijmons et al. (1990), Bio/Technol. 8, 217) harboring the NPTII selection marker under control of the 35S CaMV promoter and an expression cassette comprising the pea plastocyanin (PC) promoter and nos terminator sequences. The plastocyanin promoter present in pVDH275 has been described by Pwee & Gray (1993) Plant J. 3, 437. This promoter has been transferred to the binary vector using PCR amplification and primers which contain suitable cloning sites.

Cloning of the E. Coli otsB Gene and Construction of pMOG100 (35S CaMV TPP)

A set of oligonucleotides, TPP I (5′ CTCAGATCTGGCCACAAA 3′) (SEQ ID NO: 56) and TPP II (5′ GTGCTCGTCTGCAGGTGC 3′) (SEQ ID NO: 57), was synthesized complementary to the sequence of the E. coli TPP gene (SEQ ID NO: 3). These primers were used to PCR amplify a DNA fragment of 375 bp harboring the 3′ part of the coding region of the E. coli TPP gene, introducing a PstI site 10 bp down-stream of the stop codon, using pMOG748 (WO 95/01446) as a template. This PCR fragment was digested with BglII and PstI and cloned into pMG445 (EP 0 449 376 A2 example 7a) and linearized with BglII and PstI. The resulting vector was digested with PstI and HindIII and a PotPiII terminator was inserted (see construction pMOG845). The previous described vector was digested with BglII and HindIII, the resulting 1325 by fragment was isolated and cloned together with the 5′TPP PCRed fragment digested with SmaI and BglII into pUC18 linearized with SmaI and HindIII. The resulting vector was called pTCV124. This vector was linearized with EcoRI and SmaI and used to insert the 35S CaMV promoter (a 850 bp EcoRI-‘NcoI’ (the NcoI site was made blunt by treatment with mungbean nuclease) fragment isolated from pMOG18 containing the 35S CaMV double enhancer promoter). This vector was called pTCV 127. From this vector a 2.8 kb EcoRI-HindIII fragment was isolated containing the complete 35S TPP expression cassette and cloned in binary vector pMOG800 resulting in vector pMOG1010.

Construction of pVDH321, Plastocyanin (PC) TPP

The BamHI site of plasmid pTCV124 was removed by BamHI digestion, filling-in and subsequent religation. Subsequent digestion with HindIII and EcoRI yields a DNA fragment comprising the TPP coding region and the PotPiII terminator. BamHI linkers were added and the resulting fragment was inserted in the plant binary expression vector pVDH275 (digested with BamHI) yielding pVDH321.

Construction of a Patatin TPP Expression Vector

Similar to the construction of the patatin TPS expression vector (see construction of pMOG845), a patatin TPP expression vector was constructed yielding a binary vector (pMOG1128) which, after transformation, can effectuate expression of TPP in a tuber-specific manner.

Construction of Other Expression Vectors

Similar to the construction of the above mentioned vectors, gene constructs can be made where different promoters are used, in combination with TPS, TPP or trehalase using binary vectors with the NPTII gene or the Hygromycin-resistance gene as selectable marker gene. A description of binary vector pMOG22 harboring a HPT selection marker is given in Goddijn et al. (1993) Plant J. 4, 863.

Triparental Matings

The binary vectors are mobilized in triparental matings with the E. coli strain HB 101 containing plasmid pRK2013 (Ditta et al. (1980) Proc. Natl. Acad. Sci. USA 77, 7347) into Agrobacterium tumefaciens strain MOG101 or EHA105 and used for transformation.

Transformation of Tobacco (Nicotiana tabacum Cv. SR1 or Cv, Samsun NN)

Tobacco was transformed by cocultivation of plant tissue with Agrobacterium tumefaciens strain MOG101 containing the binary vector of interest as described. Transformation was carried out using cocultivation of tobacco leaf disks as described by Horsch et al. (1985) Science 227, 1229. Transgenic plants are regenerated from shoots that grow on selection medium containing kanamycin, rooted and transferred to soil.

Transformation of Potato

Potato (Solanum tuberosum cv. Kardal) was transformed with the Agrobacterium strain EHA 105 containing the binary vector of interest. The basic culture medium was MS30R3 medium consisting of MS salts (Murashige and Skoog (1962) Physiol. Plant. 14, 473), R3 vitamins (Ooms et al. (1987) Theor. Appl. Genet. 73, 744), 30 g/l sucrose, 0.5 g/l MES with final pH 5.8 (adjusted with KOH) solidified when necessary with 8 g/l Daichin agar. Tubers of Solanum tuberosum cv. Kardal were peeled and surface sterilized by burning them in 96% ethanol for 5 seconds. The flames were extinguished in sterile water and cut slices of approximately 2 mm thickness. Disks were cut with a bore from the vascular tissue and incubated for 20 minutes in MS30R3 medium containing 1−5×10⁸ bacteria/ml of Agrobacterium EHA 105 containing the binary vector. The tuber discs were washed with MS30R3 medium and transferred to solidified postculture medium (PM). PM consisted of M30R3 medium supplemented with 3.5 mg/l zeatin riboside and 0.03 mg/l indole acetic acid (IAA). After two days, discs were transferred to fresh PM medium with 200 mg/i cefotaxim and 100 mg/l vancomycin. Three days later, the tuber discs were transferred to shoot induction medium (SIM) which consisted of PM medium with 250 mg/l carbenicillin and 100 mg/l kanamycin. After 4-8 weeks, shoots emerging from the discs were excised and placed on rooting medium (MS30R3-medium with 100 mg/l cefotaxim, 50 mg/l vancomycin and 50 mg/l kanamycin). The shoots were propagated axenically by meristem cuttings.

Transformation of Lettuce

Transformation of lettuce, Lattuca sativa cv. Evola was performed according to Curtis et al. (1994) J. Exp. Bot. 45, 1441.

Transformation of Sugarbeet

Transformation of sugarbeet, Beta vulgaris (maintainer population) was performed according to Fry et al. (1991) Third International Congress of ISPMB, Tucson USA Abstract No. 384, or according to Krens et al. (1996), Plant Sci. 116, 97.

Transformation of Lycopersicon esculentum Tomato transformation was performed according to Van Roekel et al. (1993) Plant Cell Rep. 12, 644.

Transformation of Arabidopsis

Transformation of Arabidopsis thaliana was carried out either by the method described by Clarke et al. (1992) Plant. Mol. Biol. Rep. 10, 178 or by the method described by Valvekens et al. (1988) Proc. Natl. Acad. Sci. USA, 85, 5536.

Induction of Micro-Tubers

Stem segments of in vitro potato plants harboring an auxiliary meristem were transferred to micro-tuber inducing medium. Micro-tuber inducing medium contains 1 X MS-salts supplemented with R3 vitamins, 0.5 g/l MES (final pH=5.8, adjusted with KOH) and solidified with 8 g/l Daichin agar, 60 g/l sucrose and 2.5 mg/l kinetin. After 3 to 5 weeks of growth in the dark at 24° C., micro-tubers were formed.

Isolation of Validamycin A

Validamycin A has been found to be a highly specific inhibitor of trehalases from various sources ranging from (IC₅₀) 10⁻⁶M to 10⁻¹° M (Asano et al. (1987) J. Antibiot. 40, 526; Kameda et al. (1987) J. Antibiot 40, 563). Except for trehalase, it does not significantly inhibit any α- or β-glycohydrolase activity. Validamycin A was isolated from Solacol, a commercial agricultural formulation (Takeda Chem. Indust., Tokyo) as described by Kendall et al. (1990) Phytochemistry 29, 2525. The procedure involves ion-exchange chromatography (QAE-Sephadex A-25 (Pharmacia), bed vol. 10 ml, equilibration buffer 0.2 mM Na-Pi pH 7) from a 3% agricultural formulation of Solacol. Loading 1 ml of Solacol on the column and eluting with water in 7 fractions, practically all Validamycin was recovered in fraction 4. Based on a 100% recovery, using this procedure, the concentration of Validamycin A was adjusted to 1.10⁻³ M in MS-medium, for use in trehalose accumulation tests. Alternatively, Validamycin A and B may be purified directly from Streptomyces hygroscopicus var. limoneus, as described by Iwasa et al. (1971) J. Antibiot. 24, 119, the content of which is incorporated herein by reference.

Carbohydrate Analysis

Carbohydrates were determined quantitatively by anion exchange chromatography with pulsed electrochemical detection. Extracts were prepared by extracting homogenized frozen material with 80% EtOH. After extraction for 15 minutes at room temperature, the soluble fraction is evaporated and dissolved in distilled water. Samples (25 μl) were analyzed on a Dionex DX-300 liquid chromatograph equipped with a 4×250 mm Dionex 35391 carbopac PA-1 column and a 4×50 mm Dionex 43096 carbopac PA-1 precolumn Elution was with 100 mM NaOH at 1 ml/min followed by a NaAc gradient. Sugars were detected with a pulsed electrochemical detector (Dionex, PED). Commercially available carbohydrates (Sigma) were used as a standard.

Starch Analysis

Starch analysis was performed as described in: Aman et al. (1994) Methods in Carbohydrate Chemistry, Volume X (eds. BeMiller et al.), pp 111-115.

Expression Analysis

The expression of genes introduced in various plant species was monitored using Northern blot analysis.

Trehalose-6-Phosnhate Phosphatase Assay TPP was assayed at 37° C. by measuring the production of [¹⁴C]trehalose from [¹⁴C]trehalose-6-phosphate (Londesborough and Vuorio (1991) J. of Gen. Microbiol. 137, 323). Crude extracts were prepared in 25 mM Tris, HCl pH 7.4, containing 5.5 mM MgCl₂. Samples were diluted to a protein concentration of 1 mg/ml in extraction buffer containing 1 mg/ml BSA. Standard assay mixtures (50 μl final volume) contained 27.5 mM Tris, HCl pH 7.4, 5.5 mM MgCl₂, 1 mg/ml BSA and 0.55 mM T-6-P (specific activity 854 cpm/nmol). Reactions were initiated by the addition of 5 .mu.l enzyme and terminated after 1 hour by heating for 5 minutes in boiling water. AG1-X8 (formate) anion-exchange resin (BioRad) was added and the reaction mixtures were centrifuged after 20 minutes of equilibration at room temperature. The radioactivity in the supernatant of the samples (400 μl) was measured by liquid scintillation counting.

Preparation of Plant Extracts for Hexokinase Assays

Frozen plant material was grinded in liquid nitrogen and homogenized for 30 seconds with extraction buffer (EB: 100 mM HEPES pH7.0 (KOH), 1% (w/v) PVP, 5 mM MgCl₂, 1.5 mM EDTA, 0.1% v/v β-MeOH) including Proteinase Inhibitors Complete (Boehringer Mannheim). After centrifugation, proteins in the supernatant were precipitated using 80% ammoniumsulphate and dissolved in Tris-HCl pH 7.4 and the extract was dialyzed overnight against 100 mM Tris-HCl pH 7.4. Part of the sample was used in the hexokinase assay.

Hexokinase Assay

Hexokinase activity was measured in an assay containing 0.1 M Hepes-KOH pH 7.0, 4 mM MgCl₂, 5 mM ATP, 0.2 mM NADP⁺, 10 U/ml Creatine Phosphate Kinase (dissolved in 50% glycerol, 0.1% BSA, 50 mM Hepes pH 7.0), 3.5 mM Creatine Phosphate, 7 U/ml Glucose-6-Phosphate Dehydrogenase and 2 mM Glucose by measuring the increase in OD at 340 nm at 25° C.

When 2 mM Fructose was used instead of glucose as substrate for the hexokinase reaction, 3.8 U/ml Phosphoglucose Isomerase was included. Alternatively, a hexokinase assay as described by Gancedo et al. (1977) J. Biol. Chem. 252, 4443 was used.

Example 1 Expression of the E. Coli otsA Gene (TPS) in Tobacco and Potato

Transgenic tobacco plants were generated barbouring the otsA gene driven by the de35SCaMV promoter (pMOG799) or the plastocyanin promoter (pVDH318).

Transgenic potato plants were generated harboring the otsA gene driven by the potato tuber-specific patatin promoter (pMOG845).

Tobacco leaf discs were transformed with the binary vector pMOG799 using Agrobacterium tumefaciens. Transgenic shoots were selected on kanamycin.

Leaves of some soil-grown plants did not fully expand in lateral direction, leading to a lancet-shaped morphology (FIG. 31).

Furthermore, apical dominance was reduced resulting in stunted growth and formation of several axillary shoots. Seven out of thirty-two plants showed severe growth reduction, reaching plant heights of 4-30 cm at the time of flowering (Table 1).

TABLE 1 Trehalose accumulation in leaf samples of otsA transgenic tobacco plants and their plant length at the time of flowering. trehalose height plant-line mg · g fresh weight cm controls 0.00 60-70 799-1 0.04 ND 799-3 0.02 10 799.5 0.08  4 799-15 0.055 30 799-24 0.02 12 799-26 0.05 25 799-32 0.055 30 799-40 0.11 25 ND: not determined

Control plants reached lengths of 60-70 cm at the time of flowering. Less seed was produced by transgenic lines with the stunted growth phenotype. Northern blot analysis confirmed that plants having the stunted growth phenotype expressed the otsA gene from E. coli (FIG. 2). In control plants no transcript could be detected. The functionality of the introduced gene was proven by carbohydrate analyses of leaf material from 32 transgenic greenhouse-grown tobacco plants, revealing the presence of 0.02 to 0.12 mg·g⁻¹ fresh weight trehalose in plants reduced in length (Table 1) indicating that the product of the TPS-catalyzed reaction is dephosphorylated by plant phosphatases. Further proof for the accumulation of trehalose in tobacco was obtained by treating crude extracts with porcine trehalase. Prolonged incubation of a tobacco leaf extract with trehalase resulted in complete degradation of trehalose (data not shown). Trehalose was not detected in control plants or transgenic tobacco plants without an aberrant phenotype.

TABLE 1a Primary PC-TPS tobacco transformants Leaf Leaf Plant Fw/ Dry Dry Plant- tw area No. of height Leaf Axillary area matter matter/area line cm² cm² branches cm color shoots g/cm² % g/cm² ctrl. 1 8.18 349.37 1 wt 0.023 7.21 0.0017 ctrl. 2 10.5 418.89 1 wt 0.025 9.52 0.0024 ctrl. 3 9.99 373.87 1 wt 0.027 12.91 0.0035 ctrl. 4 9.91 362.92 1 wt 0.027 9.59 0.0026 ctrl. 5 9.82 393.84 1 wt 0.025 11.51 0.0029 average 0.0254 10.148 0.0026 2 8.39 290 2 105 wt 0.029 12.16 0.0035 3 9.34 296 1 123 wt 0.032 12.21 0.0039 4 8.36 254 2 130 wt many 0.033 10.05 0.0033 6 2.28 106 5 90 wt 0.022 11.40 0.0025 8 5.21 133 4 100 dark many 0.039 7.49 0.0029 10 8.08 258 2 165 dark many 0.031 12.25 0.0038 11 2.61 64 12 95 dark many 0.041 9.20 0.0038 13 2.83 92 1 150 dark many 0.031 8.48 0.0026 16 5.86 209 3 130 dark many 0.028 10.58 0.0030 17 5.15 224 2 155 wt 0.023 11.65 0.0027 18 17.2 547 1 133 wt 0.031 10.35 0.0033 19 2.13 63 4 80 dark many 0.034 11.74 0.0040 20 3.44 113 4 90 wt + Da many 0.030 8.14 0.0025 21 9.88 246 1 105 dark many 0.040 8.50 0.0034 22 13.1 409 1 135 wt 0.032 10.68 0.0034 23 2.50 73 6 55 dark many 0.034 8.80 0.0030 24 8.76 286 2 130 wt 0.031 15.07 0.0046 27 7.91 219 1 124 wt 0.036 14.41 0.0052 28 10.0 269 2 117 dark many 0.038 8.62 0.0032 29 4.17 142 1 85 dark many 0.029 10.07 0.0030 30 10.2 343 1 160 wt 0.030 9.56 0.0029 32 1.95 61 3 75 dark many 0.032 8.21 0.0026 33 2.85 96 5 95 wt + Da many 0.030 11.23 0.0033 34 8.38 244 1 123 wt 0.034 13.60 0.0047 35 5.59 173 3 126 wt 0.032 14.49 0.0047 36 3.28 84 3 100 dark many 0.039 11.28 0.0044 37 7.80 222 1 125 wt + Da many 0.035 11.28 0.0040 39 3.70 131 2 123 wt 0.028 17.84 0.0050 40 2.40 68.5 3 108 dark many 0.035 9.58 0.0034 average 0.032 11.00 0.0035

Transgenic pVDH318 transgenic tobacco plants developed stunted growth and development of small leaves which were darker green and slightly thicker than control leaves, a phenotype similar to the pMOG799 transgenic plants (Table 1a). Further analysis of these leaves showed an increased fresh and dry weight per leaf-area compared to the controls (Tables 1a and 2). The dark green leaves indicate the presence of more chlorophyll in the transgenic leaves (Table 1b). Plants transgenic for pNOG799 (35STPS) and pMCG1177 (PCTPS) were analyzed on soluble carbohydrates, chlorophyll, trehalose and starch (FIG. 32). pMOG1177 is functionally identical to pVDH318.

TABLE 1b Chlorophyll content of N. tabacum leaves (T₀) transgenic for PC-TPS Chlorophyll Sample (mg/g leaf) Control 1 0.59 PC TPS 10-1 0.75 PC TPS 10-2 0.80 PC TPS 11 0.60 PC TPS 13 0.81 PC TPS 16 0.90 PC TPS 19 0.64 PC TPS 37 0.96 Note: light conditions during growth will influence the determined levels of chlorophyll significantly. The calculated amounts of chlorophyll may thus only be compared between plants harvested and analyzed within one experiment!

TABLE 2 Fresh weight and dry weight data of leaf material transgenic for plastocyanin-TPS_(E. coli) N. tabacum cv. Samsun NN transgenic for PC-TPS Transgene Control Fresh weight (g) 0.83 0.78 Dry weight (g) 0.072 0.079 % dry matter 8.70% 10.10% FW/area   39 (139%)   28 (100%) DW/area 3.46 (121%) 2.87 (100%) area (units) 208 275

Calculation of the ratio between the length and width of the developing leaves clearly indicate that leaves of plants transgenic for PC-TPS are more lancet-shaped (Table 3).

Potato Solanum tuberosum cv. Xardal tuber discs were transformed with Agrobacterium tumefaciens EHA105 harboring the binary vector pMOG845, transgenics were obtained with transformation frequencies comparable to empty vector controls. All plants obtained were phenotypically indistinguishable from wild type plants indicating that use of a tissue specific promoter prevents the phenotypes observed in plants where a constitutive promoter drives the TPS gene. Micro-tubers were induced on stem segments of transgenic and wild-type plants cultured on microtuber-inducing medium supplemented with 10⁻³ M Validamycin A. As a control, microtubers were induced on medium without Validamycin A. Microtubers induced on medium with Validamycin A showed elevated levels of trehalose in comparison with microtubers grown on medium without Validamycin A (Table 4). The presence of small amounts of trehalose in wild-type plants indicates the presence of a functional trehalose biosynthetic pathway.

TABLE 3 Tobacco plants (cv. Samsun NN) transgenic for pVDH318 Transformant Length (cm) Width (cm) Ratio 1/w control 1 12 8 1.50 control 2 13 8.5 1.53 control 3 12 7.5 1.60 control 4 15 9 1.67 control 5 25 16 1.56 control 6 24 16.5 1.45 control 7 28 20 1.40 control 8 25 16 1.56 control 9 26 19 1.37 control 10 21 15 1.40 1318-28 16 8.5 1.88* 1318-29 11 6.5 1.69 1318-30 19 14 1.36 1318-35 19 12 1.58 1318-39 21 16.5 1.27 1318-40 14 7 2.00* 1318-34 21 13 1.62 1318-36 13.5 7 1.93* 1318-37 17 9 1.89* 1318-4 20.5 12 1.71 1318-23 14 4.5 3.78* 1318-22 27 18 1.50 1318-19 9 4 2.25* 1318-2 27 19 1.42 1318-15 11 5 2.20* 1318-10 20 13 1.54 1318-3 25 18 1.39 1318-21 17 8.5 2.00* 1318-16 20 10 2.00* 1318-6 19 10.5 1.81 1318-20 13 5 2.60* 1318-33 12 5 2.40* 1318-27 23 20 1.15 1318-11 12 5 2.40 1318-8 18.5 6.5 2.85* 1318-24 27 17 1.59 1318-13 15 7 2.14* 1318-17 24 16 1.50 1318-18 23 16.5 1.39 * typical TPS phenotypes Ratio 1/w average of controls is 1.50

TABLE 4 Trehalose (% fresh weight) +Validamycin A −Validamycin A 845-2 0.016 — 845-4 — — 845-8 0.051 — 845-11 0.015 — 845-13 0.011 — 845-22 0.112 — 845-25 0.002 — 845-28 0.109 — wild type Kardal 0.001 —

Example 2 Expression of the E. Coli otaB Gene (TPP) in Tobacco

Transgenic tobacco plants were generated harboring the otsβgene driven by the double enhanced 35SCaMV promoter (pMOG1010) and the plastocyanin promoter (pVDH321).

Tobacco plants (cv. Samsun NN) transformed with pMOG1010 revealed in the greenhouse the development of very large leaves (leaf area increased on average up to approximately 140%) which started to develop chlorosis when fully developed (FIG. 31). Additionally, thicker stems were formed as compared to the controls, in some instances leading to bursting of the stems. In some cases, multiple stems were formed (branching) from the base of the plant (Table 5). Leaf samples of plants developing large leaves revealed 5-10 times enhanced trehalose-6-phosphate phosphatase activities compared to control plants proving functionality of the gene introduced. The dry and fresh weight/cm² of the abnormal large leaves was comparable to control leaves, indicating that the increase in size is due to an increase in dry matter and not to an increased water content. The inflorescence was also affected by the expression of TPP. Plants which had a stunted phenotype, probably caused by the constitutive expression of the TPP gene in all plant parts, developed many small flowers which did not fully mature and fell off or necrotized. The development of flowers and seed setting seems to be less affected in plants which were less stunted.

TABLE 5 Tobacco plants transgenic for pMOG1010, de35S CaMV TPP Leaf Stem Height area Bleaching Fw/cm² DW/cm² Inflorescence diameter Line (cm) cm² (5-severe) Branching (g) (g) Norm./ (mm) 1 63 489 5 + 0.096 0.0031 A 13 2 90 472 3 + 0.076 0.0035 A 19 3 103 345 0 0.072 0.0023 N 16 4 90 612 4 + 0.096 0.0039 A 5, 6, 7, 8, 14 5 104 618 1 + 0.08 0.0035 N 17 6 110 658 3 + 0.078 0.0035 N/A 19 7 120 427 0 0.074 0.0037 N 18 8 90 472 2 + 0.076 0.0023 A 6, 7, 18 9 60 354 3 + 0.092 0.0031 N   9.13 10 103 342 0 0.084 0.0025 N 16 11 110 523 1 + 0.076 0.0031 A 18 12 90 533 1 + 0.098 0.0023 N   5.16 13 53 432 4 + 0.084 0.0043 A 5, 6, 6, 14 14 125 335 0 0.086 0.0023 N 17 15 85 251 0 0.094 0.0031 N 14 16 64 352 0 + 0.076 0.0028 A   9.13 17 64 267 0 0.11 0.0018 N 15 18 71 370 2 0.086 0.0032 A 5, 7, 8, 14 19 92 672 4 + 0.076 0.0034 N 16 20 21 94 517 4 + 0.07 0.0044 N 17 22 96 659 3 + 0.082 0.0031 N 17 23 110 407 0 0.082 0.0042 N 16 24 90 381 0 0.1 0.0034 A 15 25 120 535 0 0.076 0.003 N 16 26 42 511 5 0.08 0.0038 ? 15 27 100 468 0 0.086 0.0018 N 17 28 83 583 3 0.072 0.0034 N/A 17 29 27 452 5 + 0.104 0.004 ? 7, 7, 15 30 23 479 4 + 0.076 0.0027 ? 6, 6, 7, 9, 14 31 103 308 1 0.086 0.0027 N 14 32 48 286 0 0.108 0.002 N 16 33 67 539 5 + 0.102 0.0056 A 18 34 40 311 5 + 0.084 0.0051 A 7, 7, 12

TABLE 6 Primary PC-TPP tobacco transformants Leaf Leaf Plant Dry Dry Plant- fw area No. of height Leaf Fw/ matter matter/ line (g) cm² branches cm color Bleaching area % area ctrl. 1 8.18 349.37 0.023 7.213 ctrl. 2 10.5 418.89 0.025 9.524 ctrl. 3 9.99 373.87 0.027 12.913 ctrl. 4 9.91 362.92 0.027 9.586 ctrl. 5 9.82 393.84 0.025 11.507 average 0.0255 10.149 0.0026 11 11.5 338 3 114 wt 0.0340 6.43 0.0022 12 20.1 742 pale bleaching 0.0272 9.82 0.0027 14 9.61 345 1 150 wt 0.0279 11.65 0.0032 16 5.99 234 5 54 pale bleaching 0.0256 12.85 0.0033 17 9.10 314 3 105 wt 0.0290 8.79 0.0025 18 3.78 158 3 75 pale 0.0239 7.67 0.0018 19 2.98 130 1 70 pale 0.0229 10.74 0.0025 20 8.33 296 3 70 pale bleaching 0.0281 7.56 0.0021 22 11.5 460 1 117 pale bleaching 0.0251 3.03 0.0008 24 9.42 369 1 155 wt 0.0255 10.62 0.0027 25 15.9 565 1 170 wt 0.0282 9.54 0.0027 26 8.07 343 2 155 wt 0.0235 15.37 0.0036 28 11.7 411 2 65 pale bleaching 0.0286 6.90 0.0020 29 11.6 420 1 117 pale Bleaching 0.0277 3.53 0.0010 31 8.21 307 2 153 wt 0.0267 12.79 0.0034 32 4.03 175 1 70 pale 0.0230 18.86 0.0043 34 4.81 203 1 107 pale 0.0237 20.58 0.0049 35 7.86 307 3 130 pale 0.0256 11.45 0.0029 36 4.90 206 2 95 pale 0.0238 22.65 0.0054 37 13.9 475 1 135 wt 0.0293 4.82 0.0014 38 16.6 614 1 90 pale bleaching 0.0271 3.31 0.0009 39 14.9 560 1 112 wt bleaching 0.0267 6.08 0.0016 40 24.5 843 0.0292 9.80 0.0029 41 8.86 343 1 115 wt 0.0258 2.93 0.0008 42 6.93 289 1 wt 0.0240 3.32 0.0008 43 11.3 433 136 135 wt 0.0261 6.73 0.0018 44 10.0 341 2 135 wt 0.0294 6.49 0.0019 45 9.40 327 2 135 wt 0.0287 8.51 0.0024 46 9.18 284 2 115 wt 0.0323 15.69 0.0051 average 0.027 9.60 0.0025 wt = wild-type

Tobacco plants (cv. Samsun NN) transformed with pVDH321 revealed in the greenhouse a pattern of development comparable to pMOG1010 transgenic plants (Table 6).

Plants transgenic for pMOG1010 (35S-TPP) and pMOG1124 (PC-TPP) were analyzed on carbohydrates, chlorophyll, trehalose and starch FIGS. 32 A-D. For chlorophyll data see also Table 6a.

TABLE 6a Chlorophyll content of N. tabacum leaves (T₀) transgenic for PC-TPP Chlorophyll sample (mg/g leaf) Leaf phenotype control 1 1.56 wild-type control 2 1.40 wild-type control 3 1.46 wild-type control 4 1.56 wild-type control 5 1.96 wild-type PC TPP 12 0.79 bleaching PC TPP 22 0.76 bleaching PC TPP 25 1.30 wild-type PC TPP 37 0.86 wild-type PC TPP 38 0.74 bleaching Note: light conditions during growth will influence the determined levels of chlorophyll significantly. The calculated amounts of chlorophyll may thus only be compared between plants harvested and analyzed within one experiment!

Example 3 Isolation of Gene Fragments Encoding Trehalose-6-Phosphate Synthases from Selaginella legidophylla and Helianthus annuus

Comparison of the TPS protein sequences from E. coli and S. cerevisiae revealed the presence of several conserved regions. These regions were used to design degenerated primers which were tested in PCR amplification reactions using genomic DNA of E. coli and yeast as a template. A PCR program was used with a temperature ramp between the annealing and elongation step to facilitate annealing of the degenerate primers.

PCR amplification was performed using primer sets TPSdeg 1/5 and TPSdeg 2/5 using cDNA of Selaginella lepidophylla as a template.

Degenerated primers used (IUB code):

TPSdeg1: (SEQ ID NO: 7) GAY ITI ATI TGG RTI CAY GAY TAY CA TPSdeg2: (SEQ ID NO: 8) TIG GIT KIT TYY TIC AYA YIC CIT TYC C TPSdeg5: (SEQ ID NO: 9) GYI ACI ARR TTC ATI CCR TCI C

PCR fragments of the expected size were cloned and sequenced. Since a large number of homologous sequences were isolated, Southern blot analysis was used to determine which clones hybridized with Selaginella genomic DNA. Two clones were isolated, clone 8 of which the sequence is given in SEQ ID NO: 42 (PCR primer combination 1/5) and clone 43 of which the sequence is given in SEQ ID NO: 44 (PCR primer combination 2/5) which on the level of amino acids revealed regions with a high percentage of identity to the TPS genes from E. coli and yeast.

One TPS gene fragment was isolated from Helianthus annuus (sunflower) using primer combination TPSdeg 2/5 in a PCR amplification with genomic DNA of H. annuus as a template. Sequence and Southern blot analysis confirmed the homology with the TPS genes from E. coli, yeast and Selaginella. Comparison of these sequences with EST sequences (expressed sequence tags) from various organisms, see Table 6b and SEQ ID NOS 45-53 and 41, indicated the presence of highly homologous genes in rice and Arabidopsis, which supports our invention that most plants contain TPS homologous genes (FIGS. 3A and 3B).

TABLE 6b Genbank dbest ID. Accession No. Organism Function 35567 D22143 Oryza sativa TPS 58199 D35348 Caenorhabditis elegans TPS 60020 D36432 Caenorhabditis elegans TPS 87366 T36750 Saccharomyces TPS cerevisiae 35991 D22344 Oryza sativa TPS 57576 D34725 Caenorhabditis elegans TPS 298273 H37578 Arabidopsis thaliana TPS 298289 H37594 Arabidopsis thaliana TPS 315344 T76390 Arabidopsis thaliana TPS 315675 T76758 Arabidopsis thaliana TPS 317475 R65023 Arabidopsis thaliana TPS 71710 D40048 Oryza sativa TPS 401677 D67869 Caenorhabditis elegans TPS 322639 T43451 Arabidopsis thaliana TPS 76027 D41954 Oryza sativa TPP 296689 H35994 Arabidopsis thaliana TPP 297478 H36783 Arabidopsis thaliana TPP 300237 T21695 Arabidopsis thaliana TPP 680701 AA054930 Brugia malayi trehalase 693476 C12818 Caenorhabditis elegans trehalase 311652 T21173 Arabidopsis thaliana TPP 914068 AA273090 Brugia malayi trehalase 43328 T17578 Saccharomyces TPP cerevisiae 267495 H07615 Brassica napus trehalase 317331 R64855 Arabidopsis thaliana TPP 15008 T00368 Caenorhabditis elegans trehalase 36717 D23329 Oryza sativa TPP 71650 D39988 Oryza sativa TPP 147057 D49134 Oryza sativa TPP 401537 D67729 Caenorhabditis elegans trehalase 680728 AA054884 Brugia malayi trehalase 694414 C13756 Caenorhabditis elegans trehalase 871371 AA231986 Brugia malayi trehalase 894468 AA253544 Brugia malayi trehalase 86985 T36369 Saccharomyces TPP cerevisiae

Example 4 Isolation of Plant TPS Ad TPP Genes from Nicotiana tabacum

Fragments of plant TPS- and TPP-encoding cDNA were isolated using PCR on cDNA derived from tobacco leaf total RNA preparations. The column “nested” in Table 7 indicates if a second round of PCR amplification was necessary with primer set 3 and 4 to obtain the corresponding DNA fragment. Primers have been included in the sequence listing (Table 7). Subcloning and subsequent sequence analysis of the DNA fragments obtained with the primer sets mentioned revealed substantial homology to known TPS genes (FIGS. 4 & 5).

TABLE 7 Amplification of plant derived TPS and TPP cDNAs TPS-cDNA primer 1 primer 2 nested primer 3 primer 4 “825” bp Tre-TPS-14 Deg 1 No SEQ ID NO SEQ ID NO SEQ ID NO 22 & 23 30 7 “840” bp Tre-TPS-14 Tre-TPS-12 Yes Tre-TPS-13 Deg 5 SEQ ID NO SEQ ID NO SEQ ID NO SEQ ID NO SEQ ID NO 18 & 19 30 31 32 9 “630” bp Tre-TPS-14 Tre-TPS-12 Yes Deg 2 Deg 5 SEQ ID NO SEQ ID NO SEQ ID NO SEQ ID NO SEQ ID NO 20 & 21 30 31 8 9 TPP-cDNA primer 1 primer 2 nested “723” bp Tre-TPP-5 Tre-TPP-16 No SEQ ID NO 16 & 17 SEQ ID NO 35 SEQ ID NO 38 “543” bp Tre-TPP-7 Tre-TPP-16 No SEQ ID NO 14 SEQ ID NO 36 SEQ ID NO 38 “447” bp Tre-TPP-11 Tre-TPP-16 No SEQ ID NO 12 SEQ ID NO 37 SEQ ID NO 38

Example 5 Isolation of a Bipartite TPS/TPP Gene from Helianthus annuus and Nicotiana tabacum

Using the sequence information of the TPS gene fragment from sunflower (Helianthus annuus), a full length sunflower TPS clone was obtained using RACE-PCR technology.

Sequence analysis of this full length clone and alignment with TPS2 from yeast (FIG. 6) and TPS and TPP encoding sequences indicated the isolated clone encodes a TPS/TPP bipartite enzyme (SEQ ID NO: 24, 26 and 28). The bipartite clone isolated (pMOG1192) was deposited at the Central Bureau for Strain collections under the rules of the Budapest treaty with accession number CBS692.97 at Apr. 21, 1997. Subsequently, we investigated if other plant species also contain TPS/TPP bipartite clones. A bipartite TPS/TPP cDNA was amplified from tobacco. A DNA product of the expected size (i.e. 1.5 kb) was detected after PCR with primers TPS deg1/TRE-TPP-16 and nested with TPS deg2/TRE-TPP-15 (SEQ ID NO: 33). An identical band appeared with PCR with TPS deg1/TRE-TPP-6 (SEQ ID NO: 34) and nested with TPS deg2/TRE-TPP-15. The latter fragment was shown to hybridize to the sunflower bipartite cDNA in a Southern blot experiment. Additionally, using computer database searches, an Arabidopsis bipartite clone was identified (SEQ ID NO: 39)

Example 6 Expression of Plant Derived TPS Genes in Plants

Further proof for the function of the TPS genes from sunflower and Selaginella lepidophylla was obtained by isolating their corresponding full-length cDNA clones and subsequent expression of these clones in plants under control of the 35S CaMV promoter. Accumulation of trehalose by expression of the Seliganella enzyme has been reported by Zentella and Iturriaga (1996) (Plant Physiol. 111. Abstract 88).

Example 7 Genes Encoding TPS and TPP from Monocot Species

A computer search in Genbank sequences revealed the presence of several rice EST-sequences homologous to TPS 1 and TPS2 from yeast (FIG. 7) which are included in the sequence listing (SEQ ID NO: 41, 51, 52 and 53).

Example 8 Isolation Human TPS Gene

A TPS gene was isolated from human cDNA. A PCR reaction was performed on human cDNA using the degenerated TPS primers deg2 and deg5. This led to the expected TPS fragment of 0.6 kb. Sequence analysis (SEQ ID NO: 10) and comparison with the TPSyeast sequence indicated that isolated sequence encodes a homologous TPS protein (FIG. 8).

Example 9 Inhibition of Endogenous TPS Expression by Anti-Sense Inhibition

The expression of endogenous TPS genes can be inhibited by the anti-sense expression of a homologous TPS gene under control of promoter sequences which drive the expression of such an anti-sense TPS gene in cells or tissue where the inhibition is desired. For this approach, it is preferred to use a fully identical sequence to the TPS gene which has to be suppressed although it is not necessary to express the entire coding region in an anti-sense expression vector. Fragments of such a coding region have also shown to be functional in the anti-sense inhibition of gene-expression. Alternatively, heterologous genes can be used for the anti-sense approach when these are sufficiently homologous to the endogenous gene.

Binary vectors similar to pMOG845 and pMOG1010 can be used ensuring that the coding regions of the introduced genes which are to be suppressed are introduced in the reverse orientation. All promoters which are suitable to drive expression of genes in target tissues are also suitable for the anti-sense expression of genes.

Example 10 Inhibition of Endogenous TPP Expression by Anti-Sense Inhibition

Similar to the construction of vectors which can be used to drive anti-sense expression of tps in cells and tissues (Example 9), vectors can be constructed which drive the anti-sense expression of TPP genes.

Example 11 Trehalose Accumulation in Wild-Type Tobacco and Potato Plants Grown on Validamycin A

Evidence for the presence of a trehalose biosynthesis pathway in tobacco was obtained by culturing wild-type plants in the presence of 10⁻³M of the trehalase inhibitor Validamycin A. The treated plants accumulated very small amounts of trehalose, up to 0.0021% (fw). Trehalose accumulation was never detected in any control plants cultured without inhibitor. Similar data were obtained with wild-type microtubers cultured in the presence of Validamycin A. Ten out of seventeen lines accumulated on average 0.001% trehalose (fw)/(Table 4). No trehalose was observed in microtubers which were induced on medium without Validamycin A.

Example 12 Trehalose Accumulation in Potato Plants Transgenic for Astrehalase

Further proof for the presence of endogenous trehalose biosynthesis genes was obtained by transforming wild-type potato plants with a 35S CaMV anti-sense trehalase construct (SEQ ID NO: 54 and 55, pMOG1027; described in WO 96/21030). A potato shoot transgenic for pMOG1027 showed to accumulate trehalose up to 0.008% on a fresh weight basis. The identity of the trehalose peak observed was confirmed by specifically breaking down the accumulated trehalose with the enzyme trehalase. Tubers of some pMOG1027 transgenic lines showed to accumulate small amounts of trehalose (FIG. 9).

Example 13 Inhibition of Plant Hexokinase Activity by Trehalose-6-Phosphate

To demonstrate the regulatory effect of trehalose-6-phosphate on hexokinase activity, plant extracts were prepared and tested for hexokinase activity in the absence and presence of trehalose-6-phosphate.

Potato tuber extracts were assayed using fructose (FIG. 10, FIG. 11) and glucose (FIG. 11) as substrate. The potato tuber assay using 1 mM T-6-P and fructose as substrate was performed according to Gancedo et al. (1997) J. Biol. Chem. 252, 4443. The following assays on tobacco, rice and maize were performed according to the assay described in the section experimental. Tobacco leaf extracts were assayed using fructose (FIG. 12) and glucose (FIG. 12, FIG. 13) as substrate. Rice leaf extracts were assayed using fructose and glucose (FIG. 14) as substrate. Maize leaf extracts were assayed using fructose and glucose (FIG. 15) as substrate.

Example 14 Inhibition of Hexokinase Activity in Animal Cell Cultures by Trehalose-6-Phosphate

To demonstrate the regulation of hexokinase activity in animal cells, total cell extracts were prepared from mouse hybridoma cell cultures. A hexokinase assay was performed using glucose or fructose as substrate under conditions as described by Gancedo et al. (see above). Mouse hybridoma cells were subjected to osmotic shock by exposing a cell pellet to 20% sucrose, followed by distilled water. This crude protein extract was used in the hexokinase assay (50 μl) extract corresponding to ca. 200 μg protein).

TABLE 8 Inhibition of animal hexokinase activity for T-6-P Concen- Inhi- tration T6P V0 V2 bition Substrate (mM) (ODU/min) (ODU/min) (ODU/min) (%) Glucose 2 0.83 0.0204 0.0133 35 Glucose 20 0.83 0.0214 0.0141 35 Glucose 100 0.83 0.0188 0.0125 34 Fructose 20 0.23 0.0207 0.0205 1 Fructose 20 0.43 0.0267 0.0197 26 Fructose 20 0.83 0.0234 0.0151 35 Fructose 20 1.67 0.0246 0.0133 46

The data obtained clearly showed that hexokinase activity in mouse cell extracts is inhibited by trehalose-6-phosphate. The T-6-P concentration range in which this effect is noted is comparable to what has been observed in crude plant extracts. No difference is noted in the efficiency of hexokinase inhibition by trehalose-6-phosphate using glucose or fructose as substrate for the enzyme.

Example 15 Photosynthesis and Respiration of TPS and TPP Expressing Tobacco Plants

Using tobacco plants transgenic for 35S-TPP (1010-5), PC-TPS (1318-10 and 1318-37) and wild-type Samsun NN plants, effects of expression of these genes on photosynthesis and respiration were determined in leaves.

Measurements were performed in a gas exchange-experimental set-up. Velocities of gas-exchange were calculated on the basis of differences in concentration between ingoing and outgoing air using infra-red gas-analytical equipment. Photosynthesis and respiration were measured from identical leaves. From each transgenic plant, the youngest, fully matured leaf was used (upper-leaf) and a leaf that was 3-4 leaf-“stores” lower (lower-leaf).

Photosynthesis was measured as a function of the photosynthetic active light intensity (PAR) from 0-975 μmol·m⁻²s⁻¹ (200 Watt m⁻²), in four-fold at CO₂-concentrations of 350 vpm and 950 vpm.

Respiration was measured using two different time-scales. Measurements performed during a short dark-period after the photosynthesis experiments are coded RD in table 9. These values reflect instantaneous activity since respiration varies substantially during the dark-period. Therefor, the values for the entire night-period were also summed as shown in Table 10 (only measured at 350 vpm CO₂).

TABLE 9 Rate of photosynthesis and respiration, STD is standard deviation 350 ppm 950 ppm micromol/m²/s STD micromol/m²/s STD Upper leaf Wild-type RD 0.0826 0.048 1.016 0.142 EFF 0.060 0.004 0.087 0.004 AMAX 11.596 0.588 19.215 0.942 1010-5 RD 0.873 0.060 1.014 0.134 EFF 0.059 0.002 0.090 0.007 AMAX 12.083 1.546 18.651 1.941 1318-10 RD 0.974 0.076 1.078 0.108 EFF 0.064 0.003 0.088 0.008 AMAX 16.261 2.538 24.154 1.854 1318-37 RD 1.067 0.140 1.204 0.116 EFF 0.061 0.002 0.084 0.011 AMAX 16.818 2.368 25.174 2.093 Lower leaf Wild-type RD 0.0438 0.079 0.526 0.112 EFF 0.068 0.002 0.085 0.004 AMAX 6.529 1.271 11.489 1.841 1010-5 RD 0.455 0.068 0.562 0.118 EFF 0.064 0.002 0.085 0.006 AMAX 8.527 0.770 13.181 1.038 1318-10 RD 0.690 0.057 0.828 0.086 EFF 0.064 0.008 0.085 0.005 AMAX 11.562 1.778 20.031 1.826 1318-37 RD 0.767 0.033 0.918 0.099 EFF 0.073 0.006 0.103 0.004 AMAX 13.467 1.818 19.587 1.681

TABLE 10 Respiration during 12 hour dark period (mmol CO₂) Upper leaf STD Lower leaf STD Wild-type 25.17 0.82 13.19 1.98 1010-5 30.29 5.09 13.08 1.52 1318-10 28.37 4.50 20.47 0.87 1318-37 32.53 2.01 17.7 1.03

In contrast to the respiration in the upper-leaves, in lower leaves the respiration of TPS transgenic plants is significantly higher than for wild-type and TPP plants (Table 10) indicating a higher metabolic activity. The decline in respiration during aging of the leaves is significantly less for TPS transgenic plants.

Also, the photosynthetic characteristics differed significantly between on the one hand TPS transgenic plants and on the other hand TPP transgenic and wild-type control plants. The AMAX values (maximum of photosynthesis at light saturation), efficiency of photosynthesis (EFF) and the respiration velocity during a short dark-period after the photosynthetic measurements (RD) are shown in table 9. On average, the upper TPS leaves had a 35% higher AMAX value compared to the TPP and wild-type leaves. The lower leaves show even a higher increased rate of photosynthesis (88%).

To exclude that differences in light-absorption were causing the different photosynthetic rates, absorption values were measured with a SPAD-502 (Minolta). No significant differences in absorption were measured (Table 11).

TABLE 11 Absorbtion values of transgenic lines Absorbtion (%) Upper-leaf Lower-leaf Wild-type Samsun NN 84 83 1010-5 84 82 1318-10 85 86 1318-37 86 86

Example 16 Chlorophyll-Fluorescence of TPS and TPP Expressing Tobacco Plants

Using tobacco plants transgenic for 35S-TPP (1010-5), PC-TPS (1318-10 and 1318-37) and wild-type Samsun NN plants, effects of expressing these genes were determined on chlorophyll fluorescence of leaf material. Two characteristics of fluorescence were measured:

1) ETE (electron transport efficiency), as a measure for the electron transport velocity and the generation of reducing power, and 2) Non-photochemical quenching, a measure for energy-dissipation caused by the accumulation of assimilates.

Plants were grown in a greenhouse with additional light of 100 μmol·m⁻²·s⁻¹ (04:00-20:00 hours). Day/night T=21° C./18° C.; R.H.±75%. During a night-period preceding the measurements (duration 16 hours), two plants of each genotype were transferred to the dark and two plants to the light (±430 μmol·m⁻²·s⁻¹, 20° C., R.H.±70%). The youngest fully matured leaf was measured. The photochemical efficiency of PSII (photosystem II) and the “non-photochemical quenching” parameters were determined as a function of increasing, light intensity. At each light intensity, a 300 sec. stabilisation time was taken. Measurements were performed at 5, 38, 236, 422 and 784 μmol·m⁻²·s⁻¹ PAR with a frequency of 3 light-flashes min⁻¹, 350 ppm CO₂ and 20% O₂. Experiments were replicated using identical plants, reversing the pretreatment from dark to light and vice versa. The fluorescence characteristics are depicted in FIG. 16.

The decrease in electron-transport efficiency (ETE) was comparable between TPP and wild-type plants. TPS plants clearly responded less to a increase of light intensity. This difference was most clear in the light pretreatment. These observations are in agreement with the “non-photochemical” quenching data. TPS plants clearly responded less to the additional supply of assimilates by light compared to TPP and wild-type plants. In the case of TPS plants, the negative regulation of accumulating assimilates on photosynthesis was significantly reduced.

Example 17 Export and Allocation of Assimilates in TPS and RPP Expressing Tobacco Plants

Using tobacco plants transgenic for 35S-TPP (1010-5) and PC-TPS (1318-37),

1) the export of carbon-assimilates from a fully grown leaf (indicating “relative source activity”, Koch (1996) Annu. Rev. Plant Physiol. Plant. Mol. Biol. 47, 509 and 2) the net accumulation of photo-assimilates in sinks (“relative sink activity”), during a light and a dark-period, were determined

Developmental stage of the plants: flowerbuds just visible. Labelling technique used: Steady-state high abundance 13C-labelling of photosynthetic products (De Visser et al. (1997) Plant Cell Environ 20, 37). Of both genotypes, 8 plants, using a fully grown leaf, were labelled with 5.1 atom % ¹³CO₂ during a light-period (10 hours), when appropriate followed by a dark-period (14 hours). After labelling, plants were split in: 1) shoot-tip, 2) young growing leaf, 3) young fully developed leaf (above the leaf being labelled), 4) young stem (above the leaf being labelled), 5) labelled leaf, 6) petiole and base of labelled leaf, 7) old, senescing leaf, 8) other and oldest leaves lower than the labelled leaf. 9) stem lower than the labelled leaf, 10) root-tips. Number, fresh and dry weight and ¹³C percentage (atom % ¹³C) of carbon were determined Next to general parameters as biomass, dry matter and number of leaves, calculated were: 1) Export of C out of the labelled leaf; 2) the relative contribution of imported C in plant parts; 3) the absolute amount of imported C in plant parts; 4) the relative distribution of imported C during a light period and a complete light and dark-period.

The biomass above soil of the TPP transgenics was 27% larger compared to the TPS transgenics (P<0.001); also the root-system of the TPP transgenics were better developed. The TPP plants revealed a significant altered dry matter distribution, +39% leaf and +10% stem biomass compared to TPS plants. TPS plants had a larger number of leaves, but a smaller leaf-area per leaf. Total leaf area per TPS plant was comparable with wild-type (0.4 m₂ plant⁻¹).

Relative Source Activity of a Fully Developed Leaf

The net export rate of photosynthates out of the labelled leaf is determined by the relative decrease of the % “new C” during the night (for TPP 39% and for TPS 56%) and by the total fixated amount present in the plant using the amount of “new C” in the plant (without the labelled leaf) as a measure. After a light period, TPP leaves exported 37% compared to 51% for TPS leaves (Table 11). In a following dark-period, this percentage increased to respectively 52% and 81%. Both methods support the conclusion that TPS transgenic plants have a significantly enhanced export rate of photosynthetic products compared to the TPP transgenic plants.

-   -   Absolute Amount of “New c”, in Plant Parts

Export by TPS transgenics was significantly higher compared to TPP transgenics. Young growing TPS leaves import C stronger compared to young growing TPP leaves.

Relative Increase of “New c” in Plant Parts: Sink-Strength

The relative contribution of “new C” to the concerning plant part is depicted in FIG. 17. This percentage is a measure for the sink-strength. A significant higher sink-strength was present in the TPS transgenics, especially in the shoot-top, the stem above and beneath the labelled leaf and the petiole of the labelled leaf.

TABLE 11 Source activity of a full grown labelled leaf: C accumulation and -export. Nett daily accumulation and export of C-assimilates in labelled leaf and the whole plant (above soil) after steady-state 13^(c)-labelling during a light period (day). N = 4: LSD values indicated the smallest significant differences for P < 0.05 Source activity grown leaf new C in new C in nett C export source leaf nett C export source leaf to plant Time Trans- (% of total during night (% of new C (% of total (end of) gene C in leaf) % of “Day” in plant) new C) Day TPS 17.8 — 48.7 51 TPP 22.6 — 63.0 37 Day + night TPS 7.8 56 16.6 81 TPP 13.8 39 48.4 52 LSD 0.05 2.4 6.1 Relative Distribution, within the Plant, of “New C” Between the Plant Parts: Relative Sink Strength

The distribution of fixed carbon between plant organs (FIG. 18) confirmed the above mentioned conclusions. TPS transgenic plants revealed a relative large export of assimilates to the shoot-top, the young growing leaf (day) and even the oldest leaf (without axillary meristems), and to the young and old stem.

Example 18 Lettuce Performance of Lettuce Plants Transgenic for PC-TPS and PC-TPP

Constructs used in lettuce transformation experiments: PC-TPS and PC-TPP. PC-TPS transgenics were rescued during regeneration by culturing explants on 60 g/l sucrose. The phenotypes of both TPS and TPP transgenic plants are clearly distinguishable from wild-type controls; TPS transgenic plants have thick, dark-green leaves and TPP transgenic plants have light-green leaves with a smoother leaf-edge when compared to wild-type plants.

The morphology of the leaves, and most prominent the leaf-edges, was clearly affected by the expression of TPS and TPP. Leaves transgenic for PC-TPS were far more “notched” than the PC-TPP transgenic leaves that had a more smooth and round morphology (FIG. 19). Leaf extracts of transgenic lettuce lines were analyzed for sugars and starch (FIGS. 20A-D).

Example 19 Sugarbeet Performance of Sugarbeet Plants Transgenic for PC-TPS and PC-TPP

Constructs used in sugarbeet transformation experiments: PC-TPS and PC-TPP. Transformation frequencies obtained with both the TPS and the TPP construct were comparable to controls. The phenotypes of both TPS and TPP transgenic plants were clearly distinguishable from wild-type controls; TPS transgenic plants had thick, dark-green leaves and TPP transgenic plants had light-green colored leaves with slightly taller petioles when compared to wild-type plants (FIG. 21). Taproot diameter was determined for all plants after ca. 8 weeks of growth in the greenhouse. Some PC-TPS transgenic lines having a leaf size similar to the control plants showed a significant larger diameter of the tap-root (FIG. 22). PC-TPP transgenic lines formed a smaller taproot compared to the non-transgenic controls. Leaf extracts of transgenic sugarbeet lines were analyzed for sugars and starch (FIGS. 20A-D).

Example 20 Arabidopsis Performance of Arabidopsis Plants Transgenic for PC-TPS and PC-TPP

Constructs used in Arabidopsis transformation experiments: PC-TPS and PC-TPP. The phenotypes of both TPS and TPP transgenic plants were clearly distinguishable from wild-type controls; TPS transgenic plants had thick, dark-green leaves and TPP transgenic plants had larger, bleaching leaves when compared to wild-type plants. Plants with high levels of TPP expression did not set seed.

Example 21 Potato Performance of Solanum tuberosum Plants Transgenic for TPS and TPP Constructs

Construct: 35S-TPS pMOG799

Plants transgenic for pMOG799 were grown in the greenhouse and tuber-yield was determined (FIG. 23). The majority of the transgenic plants showed smaller leaf sizes when compared to wild-type controls. Plants with smaller leaf-sizes yielded less tuber-mass compared to control lines (FIG. 25).

Construct: 35S-TPP pMOG1010 and PC-TPP pMOG1124

Plants transgenic for PMOG 1010 and pMOG1124 were grown in the greenhouse and tuber-yield was determined Tuber-yield (FIG. 24) was comparable or less than the wild-type control lines (FIG. 25).

Construct: PC-TPS pMOG1093

Plants transgenic for pMOG1093 were grown in the greenhouse and tuber-yield was determined A number of transgenic lines having leaves with a size comparable to wild-type (B-C) and that were slightly darker green in color yielded more tuber-mass compared to control plants (FIG. 26). Plants with leaf sizes smaller (D-G) than control plants yielded less tuber-mass.

Construct: Pat-TPP pMOG1128

Microtubers were induced in vitro on explants of pat-TPP transgenic plants. The average fresh weight biomass of the microtubers formed was substantially lower compared to the control lines.

Construct: Pat-TPS pMOG845

Plants transgenic for pMOG 845 were grown in the greenhouse and tuber-yield was determined. Three Pat-TPS lines produced more tuber-mass compared to control lines (FIG. 27).

Construct: PC TPS Pat TPS; pMOG 1129(845-11/22/28)

Plants expressing PC TPS and Pat-TPS simultaneously were generated by retransforming Pat-TPS lines (resistant against kanamycin) with construct pMOG1129, harboring a PC TPS construct and a hygromycin resistance marker gene, resulting in genotypes pMOG1129(845-11), pMOG1129(845-22) and pMOG1129(845-28). Tuber-mass yield varied between almost no yield up to yield comparable or higher then control plants (FIGS. 28A-C).

Example 22 Tobacco Performance of N. tabacum Plants Transgenic for TPS and TPP Constructs Root System

Tobacco plants transgenic for 35S TPP (pMOG1010) or 35S TPS (pMOG799) were grown in the greenhouse. Root size was determined just before flowering. Lines transgenic for pMOG1010 revealed a significantly smaller/larger root size compared to pMOG795 and non-transgenic wild-type tobacco plants.

Influence of Expressing TPS and/or TPP on Flowering

Tobacco plants transgenic for 35S-TPS, PC-TPS, 35S-TPP or PC-TPP were cultured in the greenhouse. Plants expressing high levels of the TPS gene revealed significantly slower growth rates compared to wild-type plants. Flowering and senescence of the lower leaves was delayed in these plants resulting in a stay-green phenotype of the normally senescing leaves. Plants expressing high levels of the TPP gene did not make any flowers or made aberrant, not fully developing flower buds resulting in sterility.

Influence of Expressing TPS and/or TPP on Seed Setting

Tobacco plants transgenic for 35S-TPS, PC-TPS, 35S-TPP or PC-TPP were cultured in the greenhouse. Plants expressing high levels of the TPP gene revealed poor or no development of flowers and absence of seed-setting.

Influence of Expressing TPS and/or TPP on Seed Germination

Tobacco plants transgenic for 35S TPP (pMOG11010) or PC TPP were grown in the greenhouse. Some of the transgenic lines, having low expression levels of the transgene, did flower and set seed. Upon germination of S1 seed, a significantly reduced germination frequency was observed (or germination was absent) compared to S1 seed derived from wild-type plants (Table 12).

TABLE 12 Germination of transgenic 35S-TPP seeds Rel. Seedlot Bleaching (TPPmRNA) Germination 1010-2 + 15.8 delayed 1010-3 − 5.3 delayed 1010-4 + 4.2 delayed 1010-5 + 5.2 delayed 1010-6 + 3.9 delayed 1010-7 − 2.8 delayed 1010-8 + 6.5 delayed 1010-9 + 4.6 delayed 1010-10 − 1.9 normal 1010-11 − 5.7 normal 1010-12 + 1.4 normal 1010-14 − 0.1 normal 1010-15 − 0.3 normal 1010-18 + 5.6 delayed 1010-20 + 6.4 delayed 1010-21 + 9.5 delayed 1010-22 + 8.8 not 1010-23 − 4.5 normal 1010-24 − 10.2 delayed 1010-25 − 4.7 delayed (less) 1010-27 − 4.8 normal 1010-28 + 22.1 delayed 1010-31 + 9.4 delayed (less) 1010-32 − 0.3 delayed (less) 1010-33 + 14.7 delayed Influence of Expressing TPS and/or TPP on Seed Yield

Seed-yield was determined for S1 plants transgenic for pMOG1010-5. On average, pMOG1010-5 yielded 4.9 g seed/plant (n=8) compared to 7.8 g seed/plant (n=8) for wild-type plants. The “1000-grain” weight is 0.06 g for line pMOG1010-5 compared to 0.08 g for wild-type Samsun NN. These data can be explained by a reduced export of carbohydrates from the source leaves, leading to poor development of seed “sink” tissue.

Influence of TPS and TPP Expression on Leaf Morphology

Segments of greenhouse grown PC-TPS transgenic, PC-TPP transgenic and non-transgenic control tobacco leaves were fixed, embedded in plastic and coupes were prepared to study cell structures using light-microscopy. Cell structures and morphology of cross-sections of the PC-TPP transgenic plants were comparable to those observed in control plants. Cross-sections of PC-TPS transgenics revealed that the spongy parenchyme cell-layer constituted of 7 layers of cells compared to 3 layers in wild-type and TPP transgenic plants (FIGS. 29A and B). This finding agrees with our observation that TPS transgenic plant lines form thicker and more rigid leaves compared to TPP and control plants.

Example 23 Inhibition of Cold-Sweetening by the Expression of Trehalose Phosphate Synthase

Transgenic potato plants (Solanum tuberosum cv. Kardal) were generated harboring the TPS gene under control of the potato tuber-specific patatin promoter (pMOG845; Example 1). Transgenic plants and wild-type control plants were grown in the greenhouse and tubers were harvested. Samples of tuber material were taken for sugar analysis directly after harvesting and after 6 months of storage at 4° C. Data resulting from the HPLC-PED analysis are depicted in FIG. 30.

What is clearly shown is that potato plants transgenic for TPS_(E.coli) have a lower amount of total sugar (glucose, fructose and sucrose) accumulating in tubers directly after harvesting. After a storage period of 6 months at 4° C., the increase in soluble sugars is significantly less in the transgenic lines compared to the wild-type control lines.

Example 24 Improved Performance of 358 TPS 358 TPP (pMOG851) Transgenic Tobacco Plants Under Drought Stress

Transgenic tobacco plants were engineered harboring both the TPS and TPP gene from E. coli under control of the 35S CaMV promoter. The expression of the TPS and TPP genes was verified in the lines obtained using Northern blot and enzyme activity measurements. pMOG851-2 was shown to accumulate 0.008 mg trehalose·g⁻¹ fw and pMOGB51-5 accumulated 0.09 mg trehalose·g⁻¹ fw. Expression of both genes had a pronounced effect on plant morphology and growth performance under drought stress. When grown under drought stress imposed by limiting water supply, the two transgenic tobacco lines tested, pMOGS51-2 and pMOG851-5, yielded total dry weights that were 28% (P<0.01) and 39% (P<0.001) higher than those of wild-type tobacco. These increases in dry weight were due mainly to increased leaf production: leaf dry weights were up to 85% higher for pMOG851-5 transgenic plants. No significant differences were observed under well-watered conditions.

Drought Stress Experiments

F1 seeds obtained from self-fertilization of primary transformants pMOG851-2 and pMOG851-5 (Goddijn et al. (1997) Plant Physiol. 113, 181) were used in this study. Seeds were sterilized for 10 minutes in 20% household bleach, rinsed five times in sterile water, and sown on half-strength Murashige and Skoog medium containing 10 g·L⁻¹ sucrose and 100 mg·L⁻¹ kanamycin. Wildtype SR1 seeds were sown on plates without kanamycin. After two weeks seedlings from all lines were transferred to soil (sandy loam), and grown in a growth chamber at 22° C. at approximately 100 μE·m⁻² light intensity, 14 h·d⁻¹. All plants were grown in equal amounts of soil, in 3.8 liter pots. The plants were watered daily with half-strength Hoagland's nutrient solution. The seedlings of pMOG851-2 and pMOG851-5 grew somewhat slower than the wildtype seedlings. Since we considered it most important to start the experiments at equal developmental stage, we initiated the drought stress treatments of each line when the seedlings were at equal height (10 cm), at an equal developmental stage (4-leaves), and at equal dry weight (as measured from two additional plants of each line). This meant that the onset of pMOG851-2 treatment was two days later than wildtype, and that of pMOG851-5 seven days later than wildtype. From each line, six plants were subjected to drought stress, while four were kept under well-watered conditions as controls. The wildtype tobacco plants were droughted by maintaining them around the wilting point: when the lower half of the leaves were wilted, the plants were given so much nutrient solution that the plants temporarily regained turgor. In practice, this meant supplying 50 ml of nutrient solution every three days; the control plants were watered daily to keep them at field capacity. The pMOG851-2 and pMOG851-5 plants were then watered in the exact same way as wildtype, i.e., they were supplied with equal amounts of nutrient solution and after equal time intervals as wildtype. The stem height was measured regularly during the entire study period. All plants were harvested on the same day (32 d after the onset of treatment for the wildtype plants), as harvesting the transgenic plants at a later stage would complicate the comparison of the plant lines. At the time of harvest the total leaf area was measured using a Delta-T Devices leaf area meter (Santa Clara, Calif.). In addition, the fresh weight and dry weight of the leaves, stems and roots was determined

A second experiment was done essentially in the same way, to analyze the osmotic potential of the plants. After 35 days of drought stress, samples from the youngest mature leaves were taken at the beginning of the light period (n=3).

Air-Drying of Detached Leaves

The water loss from air-dried detached leaves was measured from well-watered, four-week old pMOG851-2, pMOG851-5 and wildtype plants. Per plant line, five plants were used, and from each plant the two youngest mature leaves were detached and airdried at 25% relative humidity. The fresh weight of each leaf was measured over 32 hours. At the time of the experiment samples were taken from comparable, well-watered leaves, for osmotic potential measurements and determination of soluble sugar contents.

Osmotic Potential Measurements

Leaf samples for osmotic potential analysis were immediately stored in capped 1 ml syringes and frozen on dry ice. Just before analysis the leaf sap was squeezed into a small vial, mixed, and used to saturate a paper disc. The osmotic potential was then determined in Wescor C52 chambers, using a Wescor HR-33T dew point microvolt meter.

Chlorophyl Fluorescence

Chlorophyll fluorescence of the wildtype, pMOG851-2 and pMOG851-5 plants was measured for each plant line after 20 days of drought treatment, using a pulse modulation (PAM) fluorometer (Walz, Effeltrich, Germany). Before the measurements, the plants were kept in the dark for two hours, followed by a one-hour light period. Subsequently, the youngest mature leaf was dark-adapted for 20 minutes. At the beginning of each measurement, a small (0.05 μmol m⁻² s⁻¹ modulated at 1.6 KHz) measuring light beam was turned on, and the minimal fluorescence level (F₀) was measured. The maximal fluorescence level (F_(m)) was then measured by applying a: saturation light pulse of 4000 μmol m⁻² s⁻¹, 800 ms in duration. After another 20 s, when the signal was relaxed to near F₀, brief saturating pulses of actinic light (800 ms in length, 4000 μmol m⁻² s⁻¹) were given repetitively for 30 s with 2 s dark intervals. The photochemical (q_(Q)) and non-photochemical (q_(E)) quenching components were determined from the fluorescence/time curve according to Bolhar-Nordenkampf and Oquist (1993). At the moment of measurement, the leaves in question were not visibly wilted. Statistical data were obtained by one-way analysis of variance using the program Number Cruncher Statistical System (Dr. J. L. Hintze, 865 East 400 North, Kaysville, Utah 84037, USA).

Chlorophyll fluorescence analysis of drought-stressed plants showed a higher photochemical quenching (q_(Q)) and a higher ratio of variable fluorescence over maximal fluorescence (F_(v)/F_(m)) in pMOG851-5, indicating a more efficiently working photosynthetic machinery (Table 13).

TABLE 13 Chlorophyll fluorescence parameters of wild-type (wt) and trehalose-accumulating (pMOG851-2, pMOG851-5) transgenic tobacco plants. P (probability) values were obtained from ANOVA tests analyzing differences per plant line between plants grown under well-watered (control) or dry conditions, as well as differences between each of the transgenic lines and WT, grown under well-watered or dry conditions. 8-51- WT pMOG851-1 pMOG851-5 2/WT 815-5 F_(m) control 174.4 180.4 175.6 ns ns dry 151.5 155.7 167.8 ns 0.0068 P(ctrl. 0.0004 0.0000 ns dry) F_(v) control 134.6 143.3 142.8 ns ns dry 118.4 122.1 135.6 ns 0.0011 P (ctrl. 0.006 0.0000 ns dry) F_(v)/ control 0.771 0.794   0.813 0.059 0.0052 F_(m) dry 0.782 0.784   0.809 ns 0.0016 P (ctrl. Ns Ns Ns dry) q_(E) control 15.2 23.8  29.9 0.259 0.0085 dry 25.4 21.6  23.5 ns ns P (ctrl. 0.048 ns ns dry) q_(Q) control 91.3 92.4  90.4 ns ns dry 73.69 78.5  92.75 ns 0.0005 P (ctrl. 0.005 0.006 ns dry) F_(m): maximal fluorescence; F_(v): variable fluorescence (F_(m)-F₀): q_(Q): photochemical quenching: q_(E): non-photochemical quenching. F_(m), F_(v) are expressed in arbitrary units (chart mm).

Carbohydrate Analysis

At the time of harvest, pMOG851-5 plants contained 0.2 mg·g⁻¹ dry weight trehalose, whereas in pMOG851-2 and wildtype the trehalose levels were below the detection limit, under both stressed and unstressed conditions. The trehalose content in pMOG851-5 plants was comparable in stressed and unstressed plants (0.19 and 0.20 mg·g⁻¹ dry weight, respectively). Under well-watered conditions, the levels of glucose and fructose were twofold higher in pMOG851-5 plants than in wildtype. Leaves of stressed pMOG851-5 plants contained about threefold higher levels of each of the four nonstructural carbohydrates starch, sucrose, glucose and fructose, than leaves of stressed wildtype plants. In pMOG851-2 leaves, carbohydrate levels, like chlorophyll fluorescence values, did not differ significantly from those in wildtype. Stressed plants of all lines contained increased levels of glucose and fructose compared to unstressed plants.

Osmotic Potential of Drought Stressed and Control Plants

During a second, similar experiment under greenhouse conditions, the transgenic plants showed the same phenotypes as described above, and again the pMOG851-5 plants showed much less reduction in growth under drought stress than pMOG851-2 and wildtype plants. The osmotic potential in leaves of droughted pMOG851-5 plants (−1.77±0.39 Mpa) was significantly lower (P=0.017) than in wildtype leaves (−1.00±0.08 Mpa); pMOG851-2 showed intermediate values (−1.12±0.05 Mpa). Similarly, under well-watered conditions the osmotic potential of pMOG851-5 plants (−0.79±0.05 Mpa) was significantly lower (P=0.038) than that of wildtype leaves (−0.62±0.03 Mpa), with pMOG851-2 having intermediate values (−0.70±0.01 Mpa).

Airdrying of Detached Leaves

Leaves of pMOG851-2, pMOG851-5 and wildtype were detached and their fresh weight was measured over 32 hours of airdrying. Leaves of pMOG851-2 and pMOG851-5 plants lost significantly less water (P<0.05) than wildtype leaves: after 32 h leaves of pMOG851-5 and pMOG851-2 had 44% and 41% of their fresh weight left, respectively, compared to 30% for wildtype. At the time of the experiment samples were taken from comparable, well-watered leaves for osmotic potential determination and analysis of trehalose, sucrose, glucose and fructose. The two transgenic lines had lower osmotic potentials than wildtype (P<0.05), with pMOG851-5 having the lowest water potential (−0.63±0.03 Mpa), wildtype the highest (−0.51±0.02 Mpa) and pMOG851-2 intermediate (−0.57±0.04 Mpa). The levels of all sugars tested were significantly higher in leaves of pMOG851-5 plants than for wildtype leaves resulting in a threefold higher level of the four sugars combined (P=0.002). pMOG851-2 plants contained twofold higher levels of the four sugars combined (P=0.09). The trehalose levels were 0.24±0.02 mg·g⁻¹ DW in pMOG851-5 plants, and below detection in pMOG851-2 and wildtype.

Example 25 Performance of TPS and TPP Transgenic Lettuce Plant Lines Under Drought Stress

Primary TPS and TPP transformants and wild-type control plants were subjected to drought-stress. Lines transgenic for TPP reached their wilting point first, then control plants, followed by TPS transgenic plants indicating that TPS transgenic lines, as observed in other plant species, have a clear advantage over the TPP and wild-type plants during drought stress.

Example 26 Bolting of Lettuce Plants is Affected in Plants Transgenic for PC-TPS or PC-TPP

Bolting of lettuce is reduced in plants transgenic for PC-TPP (Table 14). Plant lines transgenic for PC-TPS show enhanced bolting compared to wild-type lettuce plants.

TABLE 14 Bolting of lettuce plants 3. PC- Total 1. 2. Visible 4. 5. TPP # of Normal Reduced inflo- Possible Completely lines plants bolting bolting rescence fasciation vegetative 1A 4 4 2A 3 1 2 3A 2 2 4A 5 1 1 1 2 5A 5 1 1 3 7A 1 1 8A 5 4 1 9A 5 5 10A  3 1 2 11A  5 2 3 12A  4 4 Con- 5 5 trol

Example 27 Performance of Tomato Plants Transgenic for TPS and TPP

Constructs used in tomato transformation experiments: 35S TPP, PC-TPS, PC-TPS as-trehalase, PC-TPP, E8-TPS, E8-TPP, E8TPS E8 as-trehalase. Plants transgenic for the TPP gene driven by the plastocyanin promoter and 35S promoter revealed phenotypes similar to those observed in other plants: bleaching of leaves, reduced formation of flowers or absent flower formation leading to small fruits or absence of fruits. A small number of 35S-TPP transgenic lines generated extreme large fruits. Those fruits revealed enhanced outgrow of the pericarp. Plants transgenic for the TPS gene driven by the plastocyanin promoter and 35S promoter did not form small lancet shaped leaves. Some severely stunted plants did form small dark-green leaves. Plants transgenic for PC-TPS and PC-as-trehalase did form smaller and darker green leaves as compared to control plants.

The color and leaf-edge of the 35S or PC driven TPS and TPP transgenic plants were clearly distinguishable similar to what is observed in other crops.

Plants harboring the TPS and TPP gene under control of the fruit-specific E8 promoter did not show any phenotypical differences compared to wild-type fruits. Plants transgenic for E8 TPS E8 astrehalase produced aberrant fruits with a yellow skin and incomplete ripening.

Example 28 Performance of Potato Plants Transgenic for as-Trehalase and/or TPS

Constructs: 35S as-trehalase (pMOG1027) and 35S as-trehalase Pat TPS (PMOG1027(845-11/22/28).

Plants expressing 35S as-trehalase and pat-TPS simultaneously were generated by retransforming pat-TPS lines (resistant against kanamycin) with construct pMOG1027, harboring the 35S as-trehalase construct and a hygromycin resistance marker gene, resulting in genotypes pMOG1027(845-11), pMOG1027(845-22) and pMOG1027(845-28). Microtubers were induced in vitro and fresh weight of the microtubers was determined. The average fresh weight yield was increased for transgenic lines harboring pMOG1027 (pMOG845-11/22/28). The fresh weight biomass of microtubers obtained from lines transgenic for pMOG1027 only was slightly higher then wild-type control plants. Resulting plants were grown in the greenhouse and tuber yield was determined (FIG. 33). Lines transgenic for 35S as-trehalase or a combination of 35S as-trehalase and pat-TPS yielded significantly more tuber-mass compared to control lines. Starch determination revealed no difference in starch content of tubers produced by plant lines having a higher yield (FIG. 34). A large number of the 1027(845-11/22/28) lines produced tubers above the soil out of the axillary buds of the leaves indicating a profound influence of the constructs used on plant development. Plant lines transgenic for 35S as-trehalase only did not form tubers above the soil.

Constructs: Pat as-trehalase (pMOG1028) and Pat as-trehalase Pat TPS (pMOG1028(845-11/22/28))

Plants expressing Pat as-trehalase and Pat-TPS simultaneously were generated by retransformiing Pat-TPS lines (resistant against kanamycin) with construct pMOG1028, harboring the Pat as-trehalase construct and a hygromycin resistance marker gene, resulting in genotypes pMOG1028(845-11), pMOG1028(845-22) and pMOG1028(845-28). Plants were grown in the greenhouse and tuber yield was determined (FIGS. 35A-E). A number of pMOG1028 transgenic lines yielded significantly more tuber-mass compared to control lines. Individual plants transgenic for both Pat TPS and Pat as-trehalase revealed a varying tuber-yield from almost no yield up to a yield comparable to or higher then the control-lines (FIGS. 35A-E).

Construct: PC as-trehalase (pMOG1092)

Plants transgenic for pMOG1092 were grown in the greenhouse and tuber-yield was determined Several lines formed darker-green leaves compared to controls. Tuber-yield was significantly enhanced compared to non-transgenic plants (FIG. 36).

Construct: PC as-trehalase PC-TPS (PMOG 1130)

Plants transgenic for pMOG 1130 were grown in the greenhouse and tuber-yield was determined Several transgenic lines developed small dark-green leaves and severely stunted growth indicating that the phenotypic effects observed when plants are transformed with TPS is more severe when the as-trehalase gene is expressed simultaneously (see Example 21). Tuber-mass yield varied between almost no yield up to significantly more yield compared to control plants (FIG. 37).

Example 29 Overexpression of a Potato Trehalase cDNA in N. tabacum

Construct: de35S CaMV trehalase (pMOG1078)

Primary tobacco transformants transgenic for pMOG1078 revealed a phenotype different from wild-type tobacco, some transgenics have a dark-green leaf color and a thicker leaf (the morphology of the leaf is not lancet-shaped) indicating an influence of trehalase gene-expression on plant metabolism. Seeds of selfed primary transformants were sown and selected on kanamycin. The phenotype showed to segregate in a mendelian fashion in the 51 generation.

Deposits

The following deposits were made under the Budapest Treaty. The clones were deposited at the Centraal Bureau voor Schimnelcultures, Oosterstraat 1, P.O. Box 273, 3740 AG Baarn, The Netherlands on Apr. 21, 1997 and received the following numbers:

Escherichia coli DH5alpha/pMOG1192 CBS 692.97

-   -   DH5alpha/pMOG1240 CBS 693.97     -   DH5alpha/pMOG1241 CBS 694.97     -   DH5alpha/pMOG1242 CBS 695.97     -   DH5alpha/pMOG1243 CBS 696.97     -   DH5alpha/pMOG1244 CBS 697.97     -   DH5alpha/pMOG1245 CBS 698.97

Deposited Clones:

-   pMOG1192 harbors the Helianchus annuus TPS/TPP bipartite cDNA     inserted in the multi-copy vector PGEM-T (Promega). -   pMOG1240 harbors the tobacco TPS “825” by cDNA fragment inserted in     pCRscript (Stratagene). -   pMOG1241 harbors the tobacco TPS “840” by cDNA fragment inserted in     pGEM-T (Promega). -   pMOG1242 harbors the tobacco TPS “630” by cDNA fragment inserted in     pGEM-T (Promega). -   pMOG1243 harbors the tobacco TPP “543”, by cDNA fragment inserted in     pGEM-T (Promega). -   pMOG1244 harbors the tobacco TPP “723” by cDNA fragment inserted in     a pUC18 plasmid. -   pMOG1245 harbors the tobacco TPP “447” by fragment inserted in     PGEM-T (Promega).     List of Relevant pMOG### and pVDH### Clones

1. Binary Vectors

-   pMOG23 Binary vector (ca. 10 Kb) harboring the NPTII selection     marker -   pMOG22 Derivative of pMOG23, the NPTII-gene has been replaced by the     HPT-gene which confers resistance to hygromycine -   pVDH 275 Binary vector derived from pMOG23, harbors a plastocyanin     promoter-nos terminator expression cassette. -   pMOG402 Derivative of pMOG23, a point-mutation in the NPTII-gene has     been restored, no KpnI restriction site present in the polylinker -   pMOG800 Derivative of pMOG402 with restored KpnI site in polylinker

2. TPS/TPP Expression Constructs

-   pMOG 799 35S-TPS-3′ nos'     -   pMOG 810 idem with Hyg marker -   pMOG 845 Pat-TPS-3′PotPiII     -   pMOG 925 idem with Hyg marker -   pMOG 851 35S-TPS-3′ nos 35S-TPP(atg)² -   pMOG 1010 de35S CaMV any leader TPP(gtg), PotPiII     -   pMOG 1142 idem with Hyg marker -   pMOG 1093 Plastocyanin-TPS-3′ nos     -   pMOG 1129 idem with Hyg marker -   pMOG 1177 Plastocyanin-TPS-3′PotPiII 3′ nos -   pVDH 318 Identical to pMOG1177     -   Functionally identical to pMOG1093 -   pMOG 1124 Plastocyanin-TPP(gtg) 3′PotPiII 3′ nos -   pVDH 321 Identical to pMOG1124 -   pMOG 1128 Patatin TPP(gtg) 3′PotPiII -   pMOG 1140 E8-TPS-3′ nos -   pMOG 1141 E8-TPP(gtg)-3′PotPiII

3. Trehalase Constructs

-   pMOG 1028 Patatin as-trehalase 3′PotPiII, Hygromycin resistance     marker -   pMOG 1078 de35S CaMV amv leader trehalase 3′ nos -   pMOG 1090 de35S CaMV amv leader as-trehalase 3′ nos     -   pMOG 1027 idem with Hyg marker -   pMOG 1092 Plastocyanin-as trehalase-3′ nos -   pMOG 1130 Plastocyanin-as trehalase-3′ nos Plastocyanin-TPS-3′ nos -   pMOG 1153 E8-TPS-3′ nos E8-as trehalase-3′PotPiII     1. All constructs harbour the NPTII selection marker unless noted     otherwise     2. Two types of TPP constructs have been used as described in     Goddijn et al. (1997) Plant Physio1.133, 181. 

1. Method for the stimulation of photosynthesis in a cell by increasing the intracellular availability of trehalose-6-phosphate.
 2. Method for the stimulation of sink-related activity by increasing the intracellular availability of trehalose-6-phosphate.
 3. Method for obtaining a dwarfed organism by increasing the intracellular availability of trehalose-6-phosphate.
 4. Use of compounds influencing the intracellular availability of trehalose-6-phosphate to affect the carbon flow in the glycolytic pathway.
 5. Method for the prevention of cold sweetening by increasing the intracellular availability of trehalose-6-phosphate.
 6. Method according to claim 5, characterized in that said increase of the intracellular concentration of trehalose-6-phosphate is effected by a decrease in TPP activity.
 7. Method according to claim 6, characterized in that said increase of the intracellular concentration of trehalose-6-phosphate is effected by a decrease in TPP activity.
 8. Method according to claim 8, characterized in that said increase of the intracellular concentration of trehalose-6-phosphate is effected by a decrease in TPP activity.
 9. Method for the inhibition of carbon flow in the glycolytic direction in a plant cell by increasing the intracellular availability of trehalose-6-phosphate by transformation of said plant cell with a vector comprising an antisense fragment of a trehalose-6-phosphate phosphatase (TPP) coding region, which upon expression is able to inhibit functional activity of the endogenous trehalose-6-phosphate phosphatase (TPP) gene.
 10. A cloning vector which comprises an antisense fragment of a trehalose-6-phosphate phosphatase (TPP) coding region, which upon expression is able to inhibit functional activity of the endogenous trehalose-6-phosphate phosphatase (TPP) gene in a plant cell.
 11. Plant characterized in that it or one of its ancestors is transformed with a vector comprising an antisense fragment of a trehalose-6-phosphate phosphatase (TPP) coding region, which upon expression is able to inhibit functional activity of the endogenous trehalose-6-phosphate phosphatase (TPP) gene in a cell of said plant, said plant still containing said antisense fragment. 